Microbial Biodiversity in Tasmanian Caves
MICROBIAL BIODIVERSITY
IN
TASMANIAN CAVES
Big Stalagmite, En trance Cave, Tasmania. Photograph taken by Jodie van de Kamp.
Jodie Lee van de Kamp, B.Sc. (Hons)
Submitted in fulfilment of the requirements for the degree of Doctor of Philosophy The University of Tasmania Hobart, August, 2004 Declaration I declare that this thesis contains no material which has been accepted for the award of any other degree or diploma in any tertiary institution and, to the best of my knowledge and belief, contains no material previously published or written by another person, except where due reference is made in the text of this thesis.
Jodie Lee van de Kamp
25th August 2004
2 Authority of Access
This thesis may be made available for loan and limited copying in accordance with the Copyright Act, 1968.
Jodie Lee van de Kamp
25th August 2004
3 ABSTRACT
Caves represent one of few remaining isolated planetary habitats, in terms of human impact and characterisation of microbial biodiversity. Caves are unique environments characterised by little or no light, low levels of organic nutrients, high mineral concentrations and a stable microclimate providing ecological niches for highly specialised organisms. Caves are not uniform environments in terms of geological and geochemical characteristics, as they can vary from one to the other, eg. rock type, method of formation, length, depth, number of openings to the surface, presence or absence of active streamways, degree of impact by human visitation etc. Furthermore, on a smaller scale, various microhabitats, with vast differences in community structure can exist within caves. Culture studies point to the dominance of actinomycetes in caves and reveals great taxonomic diversity within actinomycetes isolated. However it is widely accepted that only - 1 % of microbes are cultured in the laboratory. Culture-independent methods are being increasingly used to describe the composition of microbial communities and reveal significantly broader diversity than culture-based studies. Nevertheless, to date our knowledge of bacterial communities in caves is largely due to culture studies. Based on the literature available, this study was initially aimed at examining culturable vs. non-culturable diversity of actinomycetes in Entrance and Loons Caves and to gain an increased understanding of the composition of cave microbial communities employing classical isolation and advanced molecular detection methods. As the study progressed the focus evolved as it became apparent that actinomycetes dominated only very specific habitats, the dry sediment in Entrance Cave, and represented only a minor fraction of the microbial biodiversity of most other microhabitats studied. Entrance Cave dry sediments and inactive (dry) speleothems produced a higher number of actinomycete isolates compared to saturated sediments and wet formations from Entrance and Loons Caves. This was reinforced by the actinomycetes being the second most abundant group (26.8%) detected in clone analysis of the dry Entrance sediment and low abundances (4-16%) detected in saturated sediments from both Entrance and Loons Caves. Sediment phylotypes and isolates identified in this study closely resemble species associated with oligotrophic, chemolithotrophic and heterotrophic lifestyles indicating that these communities survive by utilising a combination of metabolic pathways. Bacteria involved in the nitrogen and sulfur cycles were important members of all sediment communities along with hydrogen-oxidising bacteria. Pair-wise comparisons of sediment communities demonstrated that they were more similar to each other within individual cave systems, Entrance and Loons, rather than between microhabitat types (dry vs. wet sediment) though saturated sediment from Entrance Cave did show a higher degree of similarity in community composition to Loons Cave samples than the dry sediment from Entrance Cave. Saturated sediments were dominated by oligotrophs able to fix atmospheric gases, methanotrophs and had a high proportion of rare phylotypes most likely representing new
4 lineages related to microbes detected in anaerobic, anoxic environments, but low abundances of heterotrophic microbes. Geornicrobiological activities are no longer underestimated since studies have shown that bacterial metabolism may lead to mineral precipitation or dissolution. Questions remain as to the identity of these microbes and whether they are actively involved in speleothem formation, or simply buried during mineral precipitation. Results demonstrated a marked difference between sediment communities and those associated with calcite speleothem and calcite mat samples. Results of ESEM and XRD analysis demonstrated that calcite speleothem samples ME3 and MXl are true calcite moonrnilk (mondmilch). Phylogenetic analyses and isolation results demonstrated the unique composition of the microbial communities associated with moonrnilk deposits, predominantly composed of nitrogen-fixing ~-Proteobacteria and psychrotrophic heterotrophic CFBs and to a lesser extent, heterotrophic actinomycetes. Despite XRD and ESEM analysis showing similar calcite composition and crystal morphology, phylogenetic results indicated that sample ME2 represented a very different rnicrohabitat to moonmilk samples, dominated by oligotrophic a.-Proteobacteria and heterotrophic actinomycetes composing 84.2% of the total diversity. Phylogenetic analyses and biodiversity indices reveal the striking similarities between moonmilk samples from both Entrance and Exit Caves and the uniqueness of the calcite mat in Entrance Cave. The one similarity in composition between all three calcite communities was the presence of members of the Pseudonocardineae in particular of the genus Saccharothrix, in all calcite samples. 165 rRNA gene sequencing of cave isolates detected high levels of diversity and novelty, particularly of moonrnilk isolates. A total of two putatively novel genera (within the CFBs and Actinobacteria) and 18 putatively novel species (of genera: Paracoccus, Actinoplanes I Couchioplanes, Micromonospora, Amycolatopsis, Saccharothrix, Bacillus, Paenibacillus, Methylobacterium, Porphyrobacter, Sphingomonas, Alcaligenes, Stenotrophomonas, Xanthomonas) were identified. This study represents the first reported culture-independent analysis of moonrnilk microbial communities globally and of cave sediment communities in the Southern Hemisphere. Information gained from this study and the discovery of actively growing microbial communities appearing to precipitate CaC03 provides focus for important future studies and represents a unique opportunity to examine the nature and extent of complex microbe-mineral interactions in the formation of speleothems and implications for cave management. The biodiversity described acts as a baseline for assessing environmental impacts and to identify factors influencing microbial biodiversity.
5 ACKNOWLEDGEMENTS I would like to sincerely thank the following people:
The University of Tasmania, Australian Biological Resources Study and Tasmanian Institute of Agricultural Research for funding that not only made this project possible but also allowed the work to be presented at several conferences, both nationally and internationally. National Parks and Wildlife Service, Tasmania, for in-kind support of the project including permits, data and advice.
Supervisors, Dr. David Nichols and Dr. Kevin Sanderson, for managing to capture my interest in the project, open doors for me and remain focused to the end.
Tom McMeekin, Tom Ross, Mark Brown, Adam Smolenski, Sharee McCammon, David Steele, Ralph Bottril, Susan Turner, Olivier Brassiant, Jill Rowling, Bill Cohen, Brendon Bateman and particularly John Bowman and Diana Northup, for technical expertise, excellent advice and helping me find direction when needed.
The School of Agricultural Science, particularly the fantastic Microbiology Group, for providing endless opportunities, support and so many fond and entertaining memories. Including, but not solely, Kathleen Shaw, Guy Abel, Andrew Bisset, Matthew Smith, Shane Powell, Liv McQuestin, Laurie Parkinson, Andy Measham, Jane Weatherly, Heather Haines and Jimmy Twin. Special thanks to Lyndal Mellefont, Kristen Stirling and Craig Shadbolt.
On a personal note, I am truly amazed at the overwhelming support from everyone in my life, I value that friendship more than you'll ever realise. There are so many people to thank, but special notes to, Kriss and Sarah Lawler, Mark van den Berg, Mark Jones, Nat Doran, Hill-Streeters Andy Wilson, Lee-Roy Evans and Kath Fearnley-Sander, Bee Hart, the Marauders, especially my girls and Sonya Enkleman, and for keeping me sane all these years, Tracey Brewer and Miss Holly Taylor.
My wonderful extended family for so much love, support and unquestioning faith that I will succeed. My parents, Lorraine and Peter van de Kamp, my siblings, Jas, Brad, Laura and Steven, and their partners, Megs, Bridg and Justie, who never quite understood why I stayed at 'school' for so long, but have always been there for me.
Finally, and certainly not least of all, Brendon, who always does what he can to help, has put up with me over these last few months without complaining (much©) and most of all is so full of support for the next stage of the journey. Thank you.
6 TABLE OF CONTENTS
MICROBIAL BIODIVERSITY IN TASMANIAN CAVES ...... 1
SECTION 1: ...... 9
LITERATURE REVIEW - MICROBIAL ECOLOGY OF CAVES ...... 9
1.1 MICROBIAL ECOLOGY ...... 9 1.1.1 OBJECTIVES OF MICROBIAL ECOLOGY ...... 9 1.1.2 METHODS IN MICROBIAL ECOLOGY AND TAXONOMY ...... 10 1.1.2.1 BIODIVERSITY ...... 10 1.1.2.2 COMMUNITYFlNGERPRINTING ...... 12 1.1.2.3 ECOLOGICALF'UNCTION ...... 13 1.1.3 LIMITATIONS OF METHODS ...... 16 1.2 CAVES ...... 19 1.2.l SPELEOGENESIS: CAVEFORMATION ...... 19 1.2.2 SPELEOTHEMS: CAVE DECORATION ...... 20 1.2.3 CAVE ENVIRONMENT ...... 21 1.2.4 SPELEOLOGY: CAVE STUDY ...... 22 1.3 MICROBIAL BIODIVERSITY AND ECOLOGY OF CAVES ••••••••••••••••••••••••••••••••••••••••••••••••••• 24 1.3.1 CHEMOLITHOAUTOTROPHIC SYSTEMS ...... 25 1.3.1.1 SULFUR-BASED SYSTEMS ...... 25 1.3.1.2 IRON, MANGANESE, NITRITE, AND OTHER SYSTEMS ...... 27 1.3.2 HETEROTROPHIC SYSTEMS ...... 29 1.3.3 ACTINOMYCETES IN CAVES ...... 31 1.3.3.l ACTINOBACTERIA ...... 36 1.3.3.2 ACTINOMYCETES ...... 36 1.3.3.3 ACTINOMYCETE TAXONOMY ...... 37 1.3.3.4 ACTINOMYCETE ECOLOGY ...... 38 1.4 GEOMICROBIOLOGY•••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 40 1.4. l GEOMICROBIOLOGY IN CAVES ...... 40 1.4.2 MICROBIALLY MEDIATED CAC03 PRECIPITATION ...... 43 1.4.3 MOONMILK ...... 46 1.5 SIGNIFICANCE ...... 52 1.5.1 BIODIVERSITY AND CONSERVATION VALUE ...... 52 1.5.2 BIOPROSPECTING ...... 53 1.5.3 BIOREMEDIATION ...... 54 1.5.4 BIODETERIORATION & BIOMINERALISATION PROCESSES ...... 55 1.5.4. l PALAEOLITHIC FRESCOES AND ROCK ART IN HYPOGEAN ENVIRONMENTS ...... 55 ,_ 1.5.4.2 MONUMENTS ...... 56 1.5.5 MANAGEMENT ISSUES ...... 57 ? 1.6 CONCLUSION •••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 59
7 SECTION 2: ...... 61
MICROBIAL BIODIVERSITY IN TASMANIAN CAVES ...... 61
CHAPTER 1: INTRODUCTION ...... 61 CHAPTER 2: MATERIALS AND METHODS •••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 65 2.1 SITE DESCRIPTION AND SAMPLE COLLECTION ...... 65 2.1.1 ENTRANCE-EXIT CAVE SYSTEM ······················································································ 65 2.1.2 LOONS CAVE ...... 65 2.1.3 SAMPLE COLLECTION ...... 66 2.2 MICROSCOPY ANDMINERALOGY ...... 68 2.2.1 ESEM AND X-RAY ELEMENTAL MICROANALYSIS ...... •...... •...... ~ ... 68 2.2.2 X-RAY DIFFRACTION ANALYSIS ...... 68 2.3 ISOLATION AND IDENTIFICATION OF MICROBES ...... 69 2.3. l ISOLATION AND CULTURING OF MICROBES ...... 69 2.3.2 16S RRNA GENE SEQUENCING AND PHYLOGENETIC ANALYSIS OF ISOLATES ...... 70 2.3.2. l EXTRACTION OF NUCLEIC ACIDS AND PURIFICATION ....•.....•...... 70 2.3.2.2 l 6S RRNA GENE PCR AMPLIFICATION AND PURIFICATION ...... 72 2.3.2.3 16S RRNA GENE SEQUENCING······················································································ 73 2.3.2.4 PHYLOGENETIC ANALYSIS ...... 74 2.4 MOLECULAR ANALYSIS OF SEDIMENTS AND MOONMILK ...... 75 2.4.1 EXTRACTION AND PURIFICATION OF NUCLEIC ACIDS FROM ENVIRONMENTAL SAMPLES 75 2.4.2 DGGE...... 77 2.4.3 CLONE LIBRARY ANALYSIS ····························································································· 79 2.4.4 PHYLOGENETIC AND BIODIVERSITY ANALYSIS ...... 81 CHAPTER 3: RESULTS AND DISCUSSION •••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 83 3.1 MICROSCOPY AND MINERALOGY ...... 83 3.2 METHOD DEVELOPMENT FOR CALCITE MOONMILK SAMPLES ...... 86 3.3 PHYLOGENETIC DIVERSITY OVERVIEW ...... , ...... 89 3.4 ISOLATION OF NOVEL CAVE MICROBES ...... 130 3.5 DIFFERENCES INMICROHABITATCOMMUNITY STRUCTURE ...... •...... 132 3.6 CULTURABLE VS. NON-CULTURABLE DIVERSITY ...... 138 3.7 METABOLIC/ECOLOGICAL COMPARISONS ...... 143 3.8 COMPARISON WITH OTHER CAVE ENVIRONMENTS ...... 148 CHAPTER 4: CONCLUDING REMARKS ..•.•...••...... ••...... •••...... •...... •••...... •••. 155
REFERENCES ...... 159
APPENDICES ...... 187
APPENDIX 1: MEDIA PREPARATION AND RECIPES ••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 187 MEDIA PREPARATION ...... 187 CULTURE MEDIA ...... 187 APPENDIX 2: CRYOPRESERVATION PROTOCOL•••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••••• 189
8 1.1 Microbial Ecology
SECTIONl:
LITERATURE REVIEW -MICROBIAL ECOLOGY OF CAVES
1.1 Microbial Ecology
1.1.1 Objectives of Microbial Ecology
Microbial ecology can be defined as investigating the impact of biodiversity on the
structure and function of microbial communities and the ecosystem as a whole. According to
Siering (1998) the questions directing much of the research in microbial ecology are theoretically
quite simple: i) what are the numbers and identities of microorganisms in a given sample, ii)
what are their activities and their role in ecosystem maintenance, iii) what genes are present to
encode the activities of interest, iv) are the genes being expressed (i.e., transcribed), and are
those transcripts translated and processed into active proteins, and v) what controls the rate of
transcription and translation for environmentally significant genes, and can we measure these rates in situ? Much of the recent advances in the field of microbial ecology focuses on addressing
the first question, microbial biodiversity, or, determining the identity of the organisms present
in a given community.
Microbial biodiversity is greater than the diversity of any other group of organisms.
Higher life forms rely on bacterial processes for their survival. Microorganisms are responsible
for diverse metabolic functions that affect soil, plant and animal health, for example, nutrient
cycling, organic matter formation and decomposition, soil structure formation, and plant growth
promotion. Microbial biodiversity has received particular attention in areas where industrial
applications are evident, such as for marine, medical, and food biotechnology, and where
microbial activity has important implications for Earth's climate and for the bioremediation of
polluted sites (Morris et al. 2002).
Different habitats may be characterised by a particular food source, substrate type,
micro-climate, or a combination of these. Some organisms are entirely restricted to a certain
9 1.1 Microbial Ecology habitat whilst others, referred to as cosmopolitan species, range widely across a variety of habitats. Each of these environments/microhabitats has its own characteristics which preclude
generalisations about the conditions of life in one being carried over to the others in most
instances, and which select for bacteria adapted to their own micro-climate.
Enhancing knowledge of bacterial biodiversity and ecological function provides baseline
information for conservation and sustainable development.
1.1.2 Methods in Microbial Ecology and Taxonomy
The study of microbial processes in an ecosystem is a multifaceted affair requiring
attack from many angles and utilising a wide variety of techniques (Brown, 2000). Studies of
biodiversity, characterising the composition of microbial communities in a given environment,
can largely be a descriptive endeavour, but a necessary first step in determining the nature of
biodiversity and its impact on ecological processes.
1.1.2.1 Biodiversity
Traditionally, microbial populations have been described in terms of isolating pure
cultures and investigating a wide range of phenotypic traits, many of which are related to the
practical interest in the habitat studied (eg. phenotypic characteristics of psychrophiles in
Antarctica; Nichols et al. 1993, 1999). Biodiversity studies focusing on phylogenetic or taxonomic
comparisons of microorganims reflect the historical tribulations surrounding the complexities of
defining a bacterial species and the relatedness among individuals of different genotypes
(Morris et al. 2002). Phylogenetic classification of bacteria is based on ancestral relationships
(Woese, 1987). Surprisingly the term 'phylogeny' is rarely defined precisely (Young, 2001). A
central outcome of phylogenetic classification is that taxa be monophyletic, ie. members of a
taxon under consideration share the same common ancestor. A further requirement is that taxa
sharing more recent common ancestry are considered to be more closely related to one another than they are to other taxa (Lincoln et al. 1998 in Young, 2001).
10 1.1 Microbial Ecology A study of microbial biodiversity publications by Morris & co-workers (2002), found that over the last 25 years, DNA-based characterisation techniques, in particular those based on targeted DNA sequences, have had the dominant role in studies of microbial relationships or in the search for new taxa, relative to other morphological or biochemical techniques. By the early
1980s, several studies had shown that ribosomal RNA (rRNA) held promise for phylogenetic reconstruction (Fox et al. 1980) and by the end of the decade, analysis of universally conserved nucleic acid sequences (particularly those of the small subunit rRNA gene) had become a powerful tool for microbial taxonomy, allowing identification of specific taxa on the basis of only a single gene sequence (Woese et al. 1990). In the 1990's, this approach had become the principal method of establishing phylogenetic relationships among the prokaryotes; today, it is more likely that a 165 rRNA gene sequence will be the first piece of data collected for unknown organisms, rather than a Gram stain (Lilburn & Garrity, 2004). Though rRNA methods are now commonplace it is worthwhile to quickly review the basis for this.
There are several reasons to focus on rRNAs to characterise microbial diversity and infer phylogenetic relationships. Olsen et al. (1986) summarised these as follows: i) rRNAs, as key elements of the protein-synthesising machinery, are present, and functionally and evolutionarily homologous, in all organisms, ii) rRNAs are ancient molecules, and conservation of function dictates conservation in overall structure thus, homologous rRNAs are readily identifiable by their size, iii) nucleotide sequences are also conserved allowing comparisons between different organisms and also providing convenient hybridisation targets for cloning and primer directed sequencing techniques, iv) rRNAs constitute a significant component of the cellular mass in actively growing cells (-104 ribosomes per actively growing E. coli cell; Siering, 1998) and are readily detected, isolated and sequenced from all types of organisms, v) rRNAs provide sufficient sequence information to permit statistically significant comparisons, vi) rRNA genes lack artefacts of lateral transfer between contemporaneous organisms. Thus, relationships between rRNAs reflect evolutionary relationships of the organisms. Conservation of function dictates a conservation of structure such that most of the rRNA molecule is conserved among the most divergent or organisms. Although different portions of the molecule evolve at different
11 1.1 Microbial Ecology rates resulting in hypervariable domains as well as highly conserved domains. Their resistance to evolutionary change allows the entire phylogenetic span of ancient and modern prokaryotes to be analysed simultaneously. However it has been shown that the resolution power of rRNA sequences is limited when closely related organisms that diverged at almost the same time are being examined (Woese, 1987; Fox et al. 1992).
It has been estimated that less than 1% of the total bacterial population in a given environment have been successfully isolated (Amann et al. 1995). The advent of culture independent molecular methods, especially rRNA-based techniques, led to an explosion of microbial biodiversity papers starting in the late 1980s. Much of what is known is based on distinguishing different organisms as represented by their extracted and polymerase chain reaction (PCR) amplified nucleic acids without actually culturing them or having any direct knowledge of their morphology, physiology or ecology (Kemp & Aller, 2004).
PCR amplification of nucleic acids extracted from environmental samples (eg. soil, water, ice) is at present the most powerful cultivation-independent technique. PCR facilitates the sensitive and fast detection of low amounts of specific gene fragments. This is of particular importance to this study as subsurface environments are, in general, characterised by low biomass which releases low amounts of nucleic acids upon extraction (Chandler et al. 1998).
Microbial diversity and identity can be estimated by cloning, sequencing and phylogenetic analysis of 16S rRNA amplified genes. Clone analysis, more often than not, results in sequences corresponding to previously uncharacterised and often unexpected lineages. An explosion of culture-independent studies of diversity in a wide range of microbial habitats in the past 15 years has resulted in a large database of more than 62 OOO 16S rRNA gene sequences providing a high resolution framework for phylogenetic analysis.
1.1.2.2 Community Fingerprinting
Community fingerprints, may be of use when trying to snapshot the diversity of a population or to follow changes in microbial communities that result from natural community succession, or environmental or anthropogenic perturbation. With specialised computer
12 1.1 Microbial Ecology software fingerprints can be databased and subjected to multivariate statistical analyses (eg.
Roling et al. 2000; Dunbar et al. 2001). Computer assisted analysis allows the comparison of different profiles with each other and the establishment of relationships between fingerprints and environmental conditions (Roling & van Verseveld, 2002). Thus community fingerprinting is more efficient (eg. cost, time) than more detailed clone library analysis when attempting high throughput or comparisons of several communities. Several 16S rRNA gene-based techniques have been used to fingerprint microbial communities, examples of which include, denaturing or temperature gradient gel electrophoresis (DGGE/TGGE), terminal restriction fragment length polymorphism (T-RFLP), and fluorescent in situ hybridisation (FISH).
Although relatively new, DGGE/TGGE is an increasingly popular molecular tool to analyse general patterns of community diversity in microbial ecology. In DGGE/TGGE, 16S rRNA gene fragments are separated on the basis of differences in their melting behaviour resulting in a pattern of bands on a gel (Muyzer & Smalla, 1998). Theoretically, each band represents a unique sequence and therefore a unique species (Powell et al. 2003). In T-RFLP, fluorescently labelled PCR products are digested with restriction enzymes and separated using automated sequencing technology. T-RFLP offers some important advantages over other fingerprint techniques, its resolution is higher and direct reference can be made to the 16S rRNA gene sequence database (Tiedje et al. 1999; Marsh et al. 2000). The application of FISH to microbial systems provides a way to detect and enumerate microorganisms in natural systems without culturing (eg. Giovannoni et al. 1988; Delong et al. 1989; Amann et al. 1990, 1991). FISH is a technique whereby fluorescently labelled DNA probes are annealed to a target sequence in nucleic acids of fixed cells. Probes have been used capable of identifying bacteria at varying levels of taxonomic hierarchy.
1.1.2.3 Ecological Function
By phylogenetically aligning an organism to its next nearest cultivated relative, we may shed light on the metabolic and physiological processes that are occurring (Pace, 1997). However caution is advised when considering the results of these studies as comparisons can only be
13 1.1 Microbial Ecology made when there is a high degree of sequence similarity between the identified phylotypes and known cultivated species, although even closely related organisms can show distinct physiological differences (Achenbach & Coates, 2000). For many clone sequences, no closely related cultivated species are known and until recently, linking most 16S rRNA gene information to function and ecological processes was dependent on culturing studies. Relatively new nucleic acid-based techniques, such as stable isotope probing (Radajewski et al. 2000) and bromodeoxyuridine labelling (Urbach et al. 1999), are beginning to emerge in the literature, allowing specific microbial processes and functions to be related to individual members of microbial communities in a cultivation-independent manner (Roling & van Verseveld, 2002).
These techniques rely on the synthesis of labelled DNA by microorganisms that grow in response to a specific stimulus and the subsequent separation of this labelled DNA from the pool of total DNA.
The use of biomarkers in combination with stable isotope analysis (eg. 13C) is one example of these relatively new culture-independent approaches to function analysis in microbial ecology. Biomarkers are compounds that have a biological specificity in that they are produced only by a limited group of organisms (eg. fatty acids, ether lipids). Natural abundance isotope ratios of biomarkers can be used to study organic matter sources utilised by microbes in complex ecosystems and for identifying specific groups of bacteria like methanotrophs
(Boschker & Middelburg, 2002). Addition of labelled substrates in combination with biomarker analysis enables direct identification of microbes involved in specific processes and also allows for the incorporation of bacteria into food web studies (Boschker & Niddelburg, 2002). Similarly,
FISH performed with rRNA-targeted oligonucleotide probes and microautoradiography can be used to analyse structure and function of bacterial communities. Lee et al. (1999) demonstrated the potential of this method by visualising the uptake of organic and inorganic radiolabelled substrates in probe-defined microbial populations.
To understand the role of a microorganism in a geochemical process, detection and identification of the microorganism in an environment in which the process is occurring is essential. Although demonstrating the presence of an organism in an environment where the
14 1.1 Microbial Ecology process is occurring does not mean the detected organism is important in the process of interest
(Siering, 1998). One ultimately needs to correlate the distribution and abundance of the organisms with the presence of the activity and the presence of any genes and gene products
(functional genes) involved in the process. If functional genes known to be involved in a particular process have been identified, isolated, characterised and sequenced, it is possible to use this information to develop PCR primers for amplifying the gene of interest from indigenous bacteria in natural samples. Hutchens et al. (2004) used DNA-based stable isotope probing and functional gene analysis of groundwater and mat material from Movile Cave to identify methane-assimilating populations and results suggest that aerobic methanotrophs
(Methylomonas, Methylococcus, Methylocystis/Methylosinus strains) actively convert CH4 into complex organic compounds and thus help sustain a diverse community of microbes in this closed ecosystem. This richness of methanotrophs was not revealed by RFLP analysis of the 16S rRNA gene clone library alone, demonstrating the benefits of constructing both 16S rRNA gene and functional gene libraries (Hutchens et al. 2004). Probing also increased already existing knowledge of microbial diversity in Movile Cave to include relatives of the cultivated and uncultivated members of the alpha, beta and gamma Proteobacteria, members of the
Acidobacterium division.
Amplifying and sequencing functional genes from organisms present in environmental samples allows us to investigate the distribution, evolutionary relationships, and diversity of functionally analogous genes (Siering, 1998). To prove a gene of interest is responsible for a process you must be able to detect expression of the gene in situ and correlate changes in gene expression with changes in the associated activity, for example detecting and quantifying the presence of particular messenger RNA (mRNA). This is often challenging due to the low quantities and very short lifespan of mRNA. Furthermore, gene expression studies require prior information, including transcript size and stability as well as expected levels of transcript present, which is not always available (Siering, 1998). Recent advances to increase detection sensitivities of gene expression rely on a form of PCR known as reverse transcriptase-PCR (RT
PCR). Reverse transcriptase is used to synthesise a single stranded DNA copy (cDNA) of the
15 1.1 Microbial Ecology RNA template then the complementary strand of the cDNA is synthesised and the double
stranded DNA molecule is subsequently amplified by normal PCR amplification.
1.1.3 Limitations of Methods
rRNA gene surveys have enormously extended the boundaries of microbial diversity,
but caution should be exercised when relying entirely on such an approach. In a detailed
culture-dependent survey of bacterial diversity in a wide range of deep-sea sediments, Li et al.
(1999) isolated 75 different actinomycetes; however very few actinomycete sequences were
cloned from these same samples in a later study (Colquhoun et al. 1998a,b, 2000).
The isolation of members of complex microbial communities as cultures also has
significant advantages over culture-independent molecular approaches given the inability to
identify with certainty the ecological, metabolic or physiological potential from novel molecular
sequence data (Atalan et al. 2000). It is most probable that the inability of microbiologists to
culture the majority of microbes in the laboratory results from the use of cultivation media that
does not resemble natural conditions or perhaps that some strains are interdependent (Wagner
et al. 1993). There is a trend emerging amongst microbial ecologists to continue to develop new
culture methods and media to attempt to cultivate novel taxa from so-called "unculturable"
groups of bacteria. In particular, Sait et al. (2002) and Joseph et al. (2003) had great success
culturing from Australian soils numerous phylogenetically novel microbes (the "Ellin" isolates)
belonging to previously uncultured groups using relatively simple cultivation methods.
Regardless, it is indisputable that culture-independent studies based on obtaining 16S rRNA
genes directly from the environment by broad-specificity primer PCR and cloning have greatly
improved our understanding of microbial diversity.
PCR-based surveys also have a number of recognised, inherent limitations. The quality
of extracted nucleic acids may be compromised by problems of shearing, degradation due to the
presence of contaminating nucleases, or contamination with humics or other substances known to inhibit subsequent molecular biological manipulations. Techniques must be optimised for
16 1.1 Microbial Ecology each type of environmental sample. Unfortunately, most methods for the extraction of nucleic acids from environmental samples lack a quantitative component; little data exists on the efficiencies of bacterial lysis and how these lysis efficiencies are affected by the complex matrix of biological and non-biological material within different sample types (Siering, 1998).
Unfortunately PCR does not necessarily occur in an accurate and unbiased fashion. A primary concern in amplifying 16S rRNA genes from mixed samples is the formation of chimeric sequences from the artifactual joining of 16S rRNA gene sequences of two organisms
(Liesack et al. 1991; Kopczynski et al. 1994) or from distinct copies of rRNA genes within the genome of a single organism (Wang & Wang, 1997). Such chimeric sequences occur at variable frequencies ranging from4.l-20% (Robison-Cox et al.1995) to 8.8-32% (Wang & Wang, 1997) and, therefore, should not be ignored. There are computational methods available to detect these artefacts (Robison-Cox et al. 1995; Komatsoulis & Waterman, 1997; Maidek et al. 1997), although all methods fail to detect some chimeras, especially those from closely related sequences, or misclassify non-chimeras as being chimeric. Hugenholtz & Hubert (2003) found during a recent collation within the public databases that, despite precautions taken, a surprising number of chimeric 16S rRNA gene sequences from molecular phylogenetic surveys were detectable.
However, by being vigilant and using several available methods rather than a single method, such inaccuracies can be decreased.
A separate issue is PCR bias, that genes are not equally amplified from all organisms
(Reysenbach et al. 1992; Suzuki & Giovannoni, 1996). This is one of the major drawbacks to developing quantitative PCR methods. Template bias is sometimes due to variable energetics in primer annealing and DNA denaturation due to G+C content in the template or primer DNA, in other instances causes for bias have not been identified (Suzuki & Giovannoni, 1996). Genome size and the number of different copies of rRNA genes within a given genome have also been shown to result in differential amplification of rRNA genes from mixed community DNA
(Farrelly et al. 1995). These parameters are unknown for the majority of organisms present in a given sample, thus Farrelly et al. (1995) contended that it is impossible to accurately quantify compositions of microbial communities by analysing clone libraries from amplified 16S rRNA
17 1.1 Microbial Ecology genes. Clone library analysis provides useful phylogenetic information that is reflective of community composition and relative distributions of organisms. However, small sample sizes prevent adequate representation of microbial community phylotypes because of cost and labour limitations. Community fingerprinting methods can alleviate these issues.
Although useful for quick comparisons of multiple communities, the drawbacks to fingerprint-based methods include a lack of resolution provided by gel-based separation and also difficulty in assigning phylogenetic information to the complex banding patterns that are usually obtained. With fingerprinting techniques, phylogenetic inference is most effective when only a single bacterial division or smaller group is addressed and is far less useful when the entire bacterial community is profiled (Dunbar et al. 2001). A combination of the two methods, fingerprinting and detailed clone analysis would be a more comprehensive way to study community composition.
18 1.2 Caves
1.2 Caves
Spaces below the Earth's surface range in size from microfissures to hundreds of kilometres in length and theoretically most have no natural human-accessible entrances (Curl,
1966 in Northup & Lavoie, 2001). A cave is defined as any natural space below the surface that
extends beyond the twilight zone and that is accessible to humans (Hill & Forti, 1986). Caves can
be classified in several ways, particularly by the type of rock and method of formation (Palmer,
1991). The most common types of caves are those formed in carbonate rocks. Other types of
caves are usually limited in extent and include those in gypsum, granite, quartz and sandstone.
1.2.1 Speleogenesis: Cave Fonnation
The birth of a cave system is referred to as speleogenesis (Ford & Cullingford, 1976). The
gradual solution of carbonate rocks, usually taking several millions of years, results in a wide
spectrum of landforms, collectively known as "karst" and caves are one of the most common
examples of this process. Carbonate rocks, such as limestone, are derived from the accumulation
of marine organisms (shells, corals etc) and as sediments on the sea floor. These marine
sediments consolidate over a long period of time and may be subsequently uplifted forming parts of the landmass of many regions of the world. Carbonate rocks contain carbonate minerals such as calcium carbonate (CaC03), often enriched with magnesium or iron and that are easily
dissolved by acids, even very weak solutions of acid.
Dissolution processes in carbonate rocks are due to the natural action of water. It occurs
as: i) surface water run off, flowing over impervious cap rock that lies above the more porous carbonate rock then flowing into carbonate, (swallet); ii) from a surface stream draining another rock surface further upstream, then entering the carbonate rock, (streamsink); or iii) rain water seeping through forest mulch and soils into the carbonate rock below (percolation water) (Ford
& Cullingford, 1976). These "charged" or "aggressive" waters are slightly acidic and penetrate
through points of weakness in the rock (eg. cracks, joints, bedding planes). Run off water or
19 1.2 Caves stream water also has a forceful action of erosion, corrosion and abrasion due to gravity, water mass or volume, and its sediment load of fine sands or gravels, which increases the magnitude of the dissolution process. The effect of seepage or percolating water is also ~ided by a number of factors. Rainwater contains dissolved carbon dioxide (C02) from the atmosphere forming a weak carbonic acid. This acidity is further strengthened by absorption of C02 from microbes and various humic or tannic acids from plant matter in the soil. Sulphuric acid sometimes derived from presence of sulphides in the soils, limestone or dolomite adds to the acidity of the water.
As the acidic water reaches the water table, it stays in contact with the carbonate causing further
dissolution of CaC03. This process is referred to as carbonic acid-driven speleogenesis.
Limestone caves may also be derived from a second process referred to as sulfuric acid-driven speleogenesis. Hydrogen sulfide rises along fissures until it encounters the oxygenated zone and forms sulfuric acid that dissolves the surrounding carbonate rock (Hill, 1990).
1.2.2 Speleothems: Cave Decoration
A cave, at constant temperature and invaded by percolating solutions carrying various substances, forms an excellent environment for the slow deposition of minerals (Ford &
Cullingford, 1976). One of the most commonly known aspects of caves is their visual beauty, due to their natural, internal formations, often referred to as cave decoration. These formations are secondary mineral deposits on the ceiling, floor and walls of a cave and are called
"speleothems". Most caves have enough openings to allow air movement, which evaporates some of the moisture and allows the precipitation of carbonate minerals from the seeping waters to form speleothems. Their creation depends on a number of factors: i) amount of seepage waters entering the ground above the cave, ii) type of rocks in and around the cave, iii) type of dissolved materials contained in the water as it enters the cave, and iv) the cave environment,
(eg. amount of moisture in the air, amount of air flow through the cave, cave temperature).
Formations are precipitated very slowly; it may take one hundred to one hundred and fifty years to form 2.5 cm of material and the slow growth and nearly constant conditions in
20 1.2 Caves caves results in these mineral deposits displaying spectacular crystal development (Ford &
Cullingford, 1976). The colouration of speleothems varies depending on the mineral composition of the carbonate rocks (eg. white or cream for almost pure CaC03, to yellowish or dark brown due to the presence of limonite, or red/ orange hues from dissolved iron, or blue hues from manganese). The colour variations and the various crystal configurations create the beautiful wonderland of this subterranean world.
Hill & Forti (1986) recognised 38 "official" speleothem types, with numerous subtypes and varieties, (Eg. stalactites, stalagmites, flowstones, rimstone pools and moonmilk) and described over 250 different minerals found in caves. Of special interest is moonmilk, a widely distributed, secondary formation and refers to the very hydrated white spongy /pasty or powdery masses found coating walls and speleothems in caves. It is composed of several carbonate minerals, predominately calcite. The wet pasty forms of moonmilk are so striking that some special explanation for their origin seems to be necessary, since calcite in cave environments usually has a completely different habit, hard and crystalline (Ford & Cullingford,
1976).
1.2.3 Cave Environment
Cave environments are strongly buffered against daily, seasonal and long-term climate changes occurring on the surface providing stable, sheltered and moist refuges for organisms.
The terrestrial cave environment is strongly zonal, with four major zones recognised; entrance, twilight, transition, and deep zone. The entrance zone is where the surface and underground environments meet. Beyond the entrance is the twilight zone where light still penetrates but progressively diminishes to zero. The transition zone is completely dark but the environmental effects from the surface are still felt. In the deep zone, environmental conditions are relatively stable, with fairly constant air and water temperatures (approximately the mean annual surface temperature) and the relative humidity near saturation resulting in an extremely low rate of
21 1.2 Caves evaporation (Barr & Holsinger, 1985 in Eberhard, 1999). Note that conditions may be less stable surrounding active, surface-fed streamways or passages near internal cave entrances.
The extent of the different zones depends on the size, shape and location of the entrance(s), on the-configuration of the cave passages and on the subterranean water/moisture supply (Howarth, 1988). The boundary between the transition and deep zones can be dynamic, changing on a seasonal or even daily basis, as air is pushed into, and pulled out of caves in response to changes in air density related to temperature and barometric fluctuations on the surface (Howarth, 1980). In temperate regions during summer, it is usually warmer outside the caves than inside, whereas in winter the reverse is true, generally resulting in a net movement of water vapour into caves during summer and out of caves during winter. Unlike the earth's surface, caves are not subject to the same weathering processes so what is found inside them often represents a different "snapshot" of the earth's history than would otherwise be available from the surface (http://www.speleonics.com.au; maintained by J. Rowling).
1.2.4 Speleology: Cave Study
The study of caves is called "speleology", and the study of life forms in caves,
''biospeleology". The main focus of biospeleologists is the deep, dark zone, also referred to as the hypogean environment, due to the highly specialised organisms found there. Hypogean environments are not restricted to caves, but include any system of crevices and fissures deeper than the soil layer. In caves, the hypogean domain is most conveniently open to study by man.
The hypogean domain may also be artificially penetrated for study particularly by mines and wells, both of which often yield hypogean organisms (Ford & Cullingford, 1976). These ecosystems are exposed to extreme environmental stresses and may be based on inorganic energy sources rather than sunlight. The limiting environmental characteristics of caves, little or no light, low levels of organic nutrients, high mineral concentrations and a stable microclimate, provide ecological niches for highly specialised organisms. Historically, macroscopic life was the primary source of interest for study in caves. However recently biospeleologists have turned
22 1.2 Caves their attention to the microscopic life in these systems, revealing unique microbial ecosystems
(eg. Cunningham et al. 1995; Sarbu et al. 1996; Jones 2001; Holmes et al. 2001; Schabereiter
Gurtner et al. 2002; Northup et al. 2003; Barton et al. 2004).
23 1.3 Microbial Biodiversity and Ecology of Caves
1.3 Microbial Biodiversity and Ecology of Caves
Caves are severely resource limited due to the absence of light that precludes primary production of organic material by photosynthetic organisms (Northup & Lavoie, 2001). Even so, microorganisms are widely distributed in caves and include bacteria, archaea, yeasts, fungi, and algae. Researchers proposed that the role of microbes in caves is to serve as a food source for higher trophic levels (eg. Dickson, 1979); however it was typically believed that microbes could not provide adequate energy to support a large and diverse ecosystem. In contrast, the work of
Sarbu et al. (1996) in Movile Cave, Romania, and Vlasceanu et al. (2000) in Frasassi Caves, Italy, suggest that chemoautotrophic, sulfur-based microbial communities can generate enough energy as primary producers to sustain complex cave ecosystems. These caves receive little or no surface-derived organic material, but instead microbially reduced sulfur compounds in the cave waters provide the energy for carbon dioxide fixation (Mattison et al. 1998). The work in
Movile Cave provided evidence of the first terrestrial microbial community known to be chemoautotrophically-based (Sarbu et al. 1996).
Culture-independent 165 rRNA gene sequence analyses have opened the way to study bacterial communities in environmental samples without prior cultivation and have revealed a significantly broader diversity than culture-based studies in many environments over the last 25 years (Amann et al. 1995; Head et al. 1998; Hugenholtz et al. 1998). Nevertheless, to date our knowledge of bacterial communities in caves has been largely due to culture studies (eg. Groth et al. 1999a; Laiz et al. 1999). As discussed in Section 1.1.2.3, phylogenetic analyses can be used to hint at the ecological functions of uncultivated phylotypes obtained from molecular analyses.
The recent influx of molecular analyses of cave microhabitats (Eg. Holmes et al. 2001;
Schabereiter-Gurtner et al. 2002; Northup et al. 2003; Barton et al. 2004; Chelius & Moore, 2004;
Schabereiter-Gurtner et al. 2004) have attempted to do just this; elucidating the roles of bacteria in caves, how they survive, interact with, and affect, their environment.
24 1.3 Microbial Biodiversity and Ecology of Caves 1.3.1 Chemolithoautotrophic Systems
In cave ecosystems with little or no exogenous organic input, the rich variety of redox interfaces allows primary growth of chemolithotrophic (eg. ammonium-, nitrite-, sulfur-,
manganese- or iron- oxidising) bacteria (Northup & Lavoie, 2001). Several studies of
chemolithotrophic communities have been reported in the literature and have demonstrated that
these bacteria play an important role in some cave ecosystems, acting as primary producers and
supporting growth of heterotrophic microbes (eg. Sarbu et al. 1996). These subsurface microbial
communities are based on chemolithoautotrophic energy processing where life does not depend
directly upon energy and organic carbon from photosynthesis (Stevens & McKinley, 1995).
1.3.1.1 Sulfur-based Systems
Caves containing hydrogen sulfide-rich springs represent less than 10% of all known
caves globally (Summers Engel et al. 2003). These caves serve as access points into sulfidic
groundwater aquifers, typically associated with geothermal regions and oil-field basins, which play an important role in global sulfur cycling. The microbial communities colonising sulfidic cave habitats are of particular interest due to their chemolithoautotrophic metabolism that can
sustain a high biomass and rich complex ecosystems in the subsurface (Sarbu et al. 1996; Angert et al. 1998; Hose, 1999) and their geomicrobiological impact, for example sulphuric acid-driven
speleogenesis (Engel et al. 2001; Vlasceanu et al. 2000).
Frasassi Cave, Italy, and Cueva de Villa Luz, Mexico, are sulfidic cave systems where sulfuric acid drips from the walls and deadly levels of hydrogen sulfide and carbon monoxide are emitted from springs. Yet amidst these hostile conditions a rich and diverse ecosystem of invertebrates and microorganisms are alive and well. Biofilms consisting of extreme acidophiles grow on thick crusts of gypsum and elemental sulfur on the cave walls. Clone library analysis of the Frasassi biofilm revealed at least 2 strains belonging to the genera Thiobacillus and
Sulfobacillus (Vlasceanu et al. 2000). An acid producing strain of Thiobacillus was also cultivated from the Frasassi biofilm. A defining feature of members of the Thiobacillus genus is their ability
25 1.3 Microbial Biodiversity and Ecology of Caves to gain energy from the oxidation of reduced sulfur compounds and resulting production of
sulfuric acid. Stable carbon isotope analysis revealed that the wall biofilms in Frasassi Cave are
isotopically light. Terrestrial isopods living on the cave walls showed peculiar isotopic values
markedly different from the rest of the invertebrates inhabiting the cave, implying that they are
feeding on these biofilms (Vlasceanu et al. 2000). These results imply that the cave food-web is
based on organic matter produced chemoautotrophically in situ by sulfur-oxidising microbes
forming mats that cover the bottom and the mudbanks of the streams and the walls of the cave,
similar to the microbial mats of the sulfidic springs of Movile Cave, Romania (Vlasceanu et al.
2000).
Microbially generated acid formed in the Frasassi biofilms diffuses through the gypsum
to the carbonate surface or drips from the tips of the microbial biofilms onto exposed carbonate
surfaces, causing rock dissolution (Vlasceanu et al. 2000). Summers-Engel et al. (2001)
investigated microbial diversity in mats from hydrogen sulfide rich waters and cave wall
biofilms in Cesspool Cave, Virginia, and pure cultures of Thiobacillus spp. isolated from this mat,
demonstrated the ability to corrode CaC03 (Summers-Engel et al. 2001). Corrosion of CaC03
substrata causes subsequent gypsum precipitation. Substrate dissolution can be beneficial to
microbes due to the release of nutrients such as nitrogen and phosphorus in oligotrophic
habitats (Rogers et al. 1998), but rock dissolution can also be detrimental in the case of carbonates
because of pH fluctuations, and in other rocks due to the release of toxic compounds, including
aluminium or trace elements (Engel et al. 2001).
The formation of caves in limestone bedrock was traditionally considered to be driven
by carbonic acid dissolution of carbonate, as discussed in Section 1.2.1. In contrast the formation
of Carlsbad Cavern and Lechuguilla Cave, New Mexico, and Movile Cave, Romania, is
inconsistent with this model of speleogenesis. Hill (1990) suggested that in caves where
hydrogen sulfide-rich waters are present, the production and activity of sulfuric acid might be
the primary cause of carbonate dissolution. Initially it was assumed to be a nonbiological
process, the sulfuric acid resulting from the chemical oxidation of hydrogen sulfide. Parker &
Jackson (1965), however, presented evidence that sulfuric acid production may be mediated by
26 1.3 Microbial Biodiversity and Ecology of Caves Thiobacillus spp. Since then, several studies have confirmed the significant role of acid produced by sulfur-oxidising bacteria in the dissolution of limestone suggesting that the colonisation and metabolic activity of these bacteria may be enhancing cave enlargement (Engel et al. 2001;
Vlasceanu et al. 2000).
1.3.1.2 Iron, Manganese, Nitrite, and other Systems
Microorganisms living at the interface between the host rock and cave passages can utilise reduced compounds in the host rock. Caves formed by the dissolution of limestone by carbonic acid are often enriched in iron, manganese and nitrogen and studies have yielded circumstantial evidence for chemolithoautotrophy by iron-, manganese- and nitrogen- oxidisers in these systems (Northup et al. 2000, 2003; Holmes et al. 2001). Unusual aquatic formations, mantles of mucus and biological material associated with crystalline material, in submerged passages of the Nullabor Caves, Australia contain a high proportion of phylogenetically novel sequence types and a high relative abundance (approximately 12%), of Nitrospira relatives, showing most similarity to autotrophic nitrite-oxidising bacteria (Nitrospira moscoviensis).
Holmes et al. (2001) concluded that this community structure, the presence of nitrite in the water, and the apparent absence of aquatic macrofauna, indicate biochemically novel, chemoautotrophic communities dependant on nitrite oxidation.
Lechuguilla Cave, New Mexico, is an immense ancient cave in near pristine condition, an extremely low nutrient environment with, however, sulfur, iron, and manganese deposits harbouring diverse microbial life (Northup et al. 2003). 16S rRNA gene clone analysis of corrosion residues (ferromanganese deposits) showed the presence of known iron- and manganese- oxidising/reducing bacteria including phylotypes of the genera, Hyphomicrobium,
Pedomicrobium, Leptospirillum, Stenotrophomonas and Pantoea (Northup et al. 2003). Black ferromanganese sediments in Vantului Cave, Romania, contain Hyphomicrobium spp.,
Pedomicrobium fusiforme and Pedomicrobium mangancum, known to mediate the oxidation and precipitation of manganese (Manolache & Onac, 2000). Northup et al. (2003) suggested that these diverse communities of microbes inhabiting ferromanganese deposits seem to exist by utilising
27 1.3 Microbial Biodiversity and Ecology of Caves manganese and iron from the bedrock and that the ferromanganese deposits represent, at least in part, the end-product of microbially assisted dissolution and leaching of the underlying host carbonate, and enrichment of iron and manganese through microbial oxidation (Northup et al.
2000).
Literature on oligotrophic cave communities subsisting in regions of nutrient scarcity is still sparse and the majority of these investigations have concentrated on communities sustained by a specific and measurable energy input, whether from sulfide, nitrite or surface organic input
(eg. Sarbu et al. 1996; Angert et al. 1998; Holmes et al. 2001). Barton et al. (2004) investigated microbial diversity in Fairy Cave, Colorado, looking at a wall community in the absence of observable energy sources. Their studies revealed a larger diversity in an oligotrophic environment than originally thought (phylotypes from 4 different divisions, Proteobacteria,
Actinobacteria, Cytophagales and the low G+C Gram-positive bacteria). The limestone bedrock of
Fairy Cave is almost pure CaC03, (>97.5%) with no significant reduced metal compounds available to act as electron donors and any metal ions that are present in the cave system were likely deposited by the rich mineral waters that formed the cave system (Barton et al. 2004).
Metabolic analyses suggested that the community subsists using a complex metabolic network with input from trace organics within the environment or fixation of atmospheric gases using lithotrophic metabolism (Barton et al. 2004).
A common theme was observed in cultivated relatives of the cloned phylotypes from
Fairy Cave, the fixation of atmospheric gases or the use of aromatic carbon compounds. The source of atmospheric gases is obvious, while the potential carbon sources may be the inorganic constituents of water filtering into the cave system. Previous research has suggested that cave waters contain dissolved organic matter from the soil, primarily phenolic compounds and lignin
(Saiz-Jimenez & Hermosin, 1999). These compounds can be utilised as carbon sources by many of the species related to those found in Fairy Cave. Similar mechanisms of lithotrophy have been suggested for other cave systems (eg. Cunningham et al. 1995). Northup et al. (2000) also suggested that reduced metals, such as magnesium and iron, within the limestone matrix of
28 1.3 Microbial Biodiversity and Ecology of Caves Lechuguilla Cave provide a sufficient source of electron donors for growth, which may further require the presence of atmospheric organic molecules as a carbon source.
In contrast to the molecular evidence, generally few chemolithoautotrophic bacteria in caves have been detected by cultivation as well as by PCR-based studies (Sarbu et al. 1996;
Vlasceanu et al. 2000; Engel et al. 2001; Holmes et al. 2001). As discussed in Section 1.3.1, molecular analyses revealed unexpected dominance of mostly uncultured groups, (eg. Epsilon
Proteobacteria in sulfidic springs of Lower Kane and Parker Caves). The majority of chemoautotrophic species isolated from caves belong to, the sulphur- and sulphide-oxidising genera, (Thiobacillus, Thiosphaera, Thiothrix, Thiomicrospira, Beggiatoa, Achromatium, Sulfobacillus and Thioalcalovibrio); the sulphate-reducing Desulfovibrio sp.; the iron-oxidising Leptospirrillum ferrooxidans and Thiobacillus ferrooxidans; the manganese- and iron-oxidising genus Leptothrix and nitrifiers such as Nitrobacter sp. (Schabereiter-Gurtner et al. 2002). Culture-independent analyses of Fairy Cave revealed a community distribution of phylotypes unique from previous observations in oligotrophic caves using cultivation, suggesting that many of the species identified are sufficiently adapted to the oligotrophic lifestyle and thus remain resistant to cultivation using standard techniques (Barton et al. 2004).
1.3.2 Heterotrophic Systems
Cave microbial communities usually rely on allochthonous input of organic matter transported from the surface (Groth et al. 1999a). In caves, animals and visitors can provide large amounts of organic input facilitating heterotrophic life (Hose et al. 2000; Groth & Saiz-Jimenez,
1999). Culture-dependent studies have focused on heterotrophic caves with allochtonous input of organic matter demonstrating that heterotrophic bacteria often dominate these communities
(Groth & Saiz-Jimenez, 1999). Many microbes identified from deep caves are similar to surface forms and are probably transported into caves by water, air, sediment and animals (Saiz
Jimenez 2001; Schabereiter-Gurtner et al. 2002a, b). Actinomycetes are the most abundant
29 1.3 Microbial Biodiversity and Ecology of Caves heterotrophic Gram-positive bacteria to be isolated from these caves particularly streptomycete, nocardioform and coryneform actinomycetes (Groth et al. 1999a).
Organic input may also be dissolved in the seepage/ dripping waters or as particulate organic matter carried in by active or periodic flooding of a subterranean streamway
(Schabereiter et al. 2002). High sulphate and nitrate concentrations have been found in dripping waters in Tito Bustillo and other Spanish and Italian caves (Hoyos et al. 1999) which, in addition to the concentrations of iron, manganese and other elements found in cave rocks, supports heterotrophic bacteria involved in the nitrogen, sulphur, iron and manganese cycles. Laiz et al.
(1999) investigated the microbial diversity of dripping waters of Altamira Cave, Spain. Water communities were not dominated by actinomycetes but contained low proportions of Gram positive bacteria, and were mainly composed of Gram-negative rods and cocci (Enterobacteriaceae and Vibrionaceae; genera Aeromonas and Acinetobacter). Compounding this, in an earlier study of dripping waters in Altamira Cave carried out by Somavilla et al. (1978) Bacillus and Pseudomonas appeared to be the most abundant genera, followed by Flavobacterium and Erwinia. In comparison, isolations from ceiling rock of Altamira Cave resulted mainly in Gram-positive
Streptomyces spp. The absence of culturable actinomycetes in dripping waters agrees with the observations of Kolbel-Boelke et al. (1988). They found very few actinomycetes in 60 water and sediment samples clearly demonstrating that dripping water communities are very different to those of cave rock though both are heterotrophic based systems.
Wind Cave, South Dakota, is a heterotrophic detritus-based limestone cave. Clone library analysis by Chelius & Moore (2004) illustrated that Gamma Proteobacteria and
Acidobacterza predominated water-saturated sediments in the dark zone. Furthermore, most of the microbial sequences were not related to known chemolithoautotrophs, therefore it was concluded that this particular community is likely detritus-based, where allochthonous energy and carbon are transported into the cave by infiltrating waters. Although some clones resembled sequences from other caves, they found that no cave-specific bacterial community was evident.
Clones mostly resembled those from soil, freshwater, plant associated and polluted environments (Chelius & Moore, 2004). Conversely, culture studies of the same sediments from
30 1.3 Microbial Biodiversity and Ecology of Caves Wind Cave produced representatives of only the actinomycetes and Proteobacteria (Alpha, Beta and Gamma) though clone analysis indicated that these were relatively minor components of the microbial community (Chelius & Moore, 2004). Most isolates were related to other cultivated members and sequences retrieved from soil and various polluted environments. It is important to note that Wind Cave is also a show cave, impacted by humans and lighted for tours, but this study still represents baseline data. Although in general molecular analyses reveal them as relatively minor representatives of cave communities, actinomycetes are still the most dominant group of bacteria isolated from caves (Schabereiter-Gurtner et al. 2002; Chelius & Moore, 2004).
1.3.3 Actinomycetes in Caves
Results of studies in caves of China, Korea, Northern Spain, and Southern Italy have demonstrated that actinomycetes are not only the most abundant bacteria isolated from these caves, but also reveal a great taxonomic diversity (Groth et al. 1999a,b; Groth & Saiz-Jimenez,
1999). Several new species of actinomycetes have been described from hypogean environments
(Lee et al. 2000a,b,c; Lee et al. 2001) including three new genera, Knoellia sinensis gen. nov., sp. nov. and Knoellia subterranean sp. nov, and Beutenbergia cavernae gen. nov., sp. nov., isolated from sediment sampled from Reed Flute Cave, China (Groth et al. 2002, 1999b); Hongia koreensis gen. nov., sp. nov., isolated from sediment in a gold mine cave of Korea (Lee et al. 2000). Three novel species were also described from the gold mine cave in Korea, Pseudonocardia kongjuensis sp. nov. and Saccharothrix violacea sp. nov., and S. albidocapillata comb. nov (Lee et al. 2000, 2001).
However, little has been published about the cave environments that these novel species have been described from.
Caves are not uniform environments in terms of geological and geochemical characteristics, as they can vary from one to the other, eg. rock type, method of formation, length, depth, number of openings to the surface, presence or absence of active streamways, degree of impact by human visitation etc. Furthermore, on a smaller scale, various microhabitats, with vast differences in community structure can exist within caves. It seems
31 1.3 Microbial Biodiversity and Ecology of Caves fairly widely accepted that dry cave substrate typically yields a higher proportion of actinomycetes than does dripping water and wet sediment (Kolbel-Boelke et al. 1988; Laiz et al.
1999). Somavilla et al. (1978) did not culture actinomycetes from the air of Altamira and La
Pasiega Caves, whereas Arroyo & Arroyo (1996) found actinomycetes from contact plates from the floor, walls, and ceilings of the same cave.
Limestone caves and lava tube caves often contain wonderful displays of filamentous actinomycetes that may cover entire ceilings and walls of caves giving a 'silvered' appearance.
Probably many of the discrete lichen-like colonies frequently noted on walls and formations in the dark zone may be actinomycetes of the genus Streptomyces since they often have the powdery appearance and characteristic earthy odour common to cultures of this genus. It has also been suggested that the abundant Streptomyces in caves is probably responsible for the earthy smell of caving (Caumartin, 1963 in Ford & Cullingford, 1976). Streptomyces and Nocardia are the most common, and abundant, groups isolated from caves (Arroyo & Arroyo, 1996).
Streptomyces species are particularly abundant though this may be due to their easy growth in the laboratory.
The majority of the work on actinomycetes in hypogean environments has been conducted in Altamira, Tito Bustillo, La Garma, and Llonin caves, Spain, and Grotta dei Cervi,
Italy all of which have spectacular galleries with paleolithic rock art paintings (Groth & Saiz
Jimenez, 1999; Groth et al. 1999a, 2001; Laiz et al. 1999, 2000). Groth et al. (1999a) reviewed the growth of actinomycetes on the ceiling and walls in Altamira and Tito Bustillo caves isolating approximately 350 strains. Actinomycete growth was distributed all over the caves and could be observed on the active stalactites, on upper and lower parts of the rock wall and in the cave soils. Large parts of the cave's rock surfaces were covered by macroscopic colonies (1-2 mm) visible to the naked eye and direct isolation from these colonies resulted solely in Streptomyces xanthophaeus. However culture-independent DGGE analyses detected 14 separate bands representing other species, most of them closely related to uncultured bacteria affiliated with
Proteobacteria, Acidobacteria, Cytophaga-Flavobacteria-Bacteroides group (CFBs) and Actinobacteria
(Schabereiter-Gurtner et al. 2002).
32 1.3 Microbial Biodiversity and Ecology of Caves Samples of active stalactites, wall concretions and rocks from the walls and ceilings of
the galleries have been investigated and a high number of isolates obtained. Most abundant
were genera of the actinomycetes, particularly Streptomyces especially from rock walls and soils.
Other genera isolated included Nocardia, Nocardioides, Saccharothrix, Amycolatopsis,
Brevibacterium, Rhodococcus, Aureobacterium, and members of the family Micrococcaceae. However,
in stalactites, the most abundant species isolated belonged to the low G+C Gram-positive
bacteria of the genus Bacillus, although the most conspicuous and visible to the naked eye were
actinomycetes of the genera, Agromyces, Amycolatopsis, Arthrobacter, Nocardiopsis, Rhodococcus,
and Streptomyces (Groth et al. 2001). These microorganisms are able to colonise the bare rock
surfaces utilising organics in dripping water. Apart from published novel species from caves,
most other papers characterise cave strains to the genus level only as they use morphological
and biochemical means of identification rather than phylogeny. At present it is therefore
difficult to make comparisons at the species level between cave environments.
Culture-dependent studies have focused on typical heterotrophic microbes from the
surface and have mostly come from so called "show caves" open to the public and which are
heavily impacted by humans. There is an apparent correlation between the number of visitors
and diversity of bacteria. The higher the number of visitors the higher the diversity of isolated
strains, as indicated by the data obtained in Tito Bustillo and Altamira caves (Groth et al. 1999a).
Altamira Cave revealed a great taxonomic diversity with predominant isolates belonging to
Streptomyces, Nocardia, Nocardioides, Saccharothrix, Amycolatopsis, Brevibacterium, Rhodococcus,
Aureobacterium, and members of the family Micrococcaceae (Groth et al. 1999a). Caves with
restricted access, Llonin and La Garma, yielded lower diversity. This increasing diversity is likely associated with lighting, which promotes the growth of phototrophic microorganisms,
and also the introduction of organic matter by visitors into the ecosystem (AriflO & Saiz-Jimenez
1996). Thus one could argue that it is the public nature of these caves that tend to heterotrophy
dominated by actinomycetes, rather than it being a general trend in cave systems with
allochthonous input of organic matter. However, Grotta dei Cervi shows similar colonisation patterns to Altamira Cave, in spite of the fact that this cave was discovered more recently in 1970
33 1.3 Microbial Biodiversity and Ecology of Caves (91 years later than Altamira) and visitation is restricted to scientific purposes (as in Llonin and
La Carma), the biodiversity was surprisingly high. This is perhaps due to the appreciably high
input of organic matter present in Grotta dei Cervi in the form of bat guano, promoting
heterotrophy and dominance of actinomycetes.
The study of cultivated microbes in these caves has revealed only a minor and not very
representative proportion of the cave microbial populations. Gram-positive bacteria identified in
Llonin, La Carma, Altamira, and Tito Bustillo Caves by culture-independent techniques is
relatively low (<30 %), though Gram-positive bacteria, and in particular actinomycetes were the
dominating isolates obtained from cultivation (eg. Groth & Saiz-Jimenez, 1999; Schabereiter
Gurtner et al. 2002). More recently DGGE community fingerprinting combined with
phylogenetic analyses used to investigate samples from paintings and surrounding rock in
Altamira and Tito Bustillo revealed greater taxonomic diversity detecting unknown and
unexpected bacterial groups, particularly the Proteobacteria, Acidobacteria division, CFBs,
actinomycetes, green non-sulfur bacteria and Planctomycetes. DGGE analysis of paintings in
Llonin and La Carma caves (Schabereiter-Gurtner et al. 2004) also illustrated a high biodiversity
of chemolithotrophic, as well as heterotrophic, bacteria; the most abundant groups found were
the Proteobacteria, actinomycetes and Acidobacteria. This data compared to results from Altamira
and Tito Bustillo caves revealed similarities in the bacterial community components, especially
in the high abundance of the Acidobacteria and Rhizobiaceae, and ammonia- and sulfur-oxidisers
(Schabereiter et al. 2002). Which is interesting in that Llonin and La Carma are restricted visitor
access for research purposes only whereas Altamira and Tito Bustillo are open to the public.
These studies have revealed diverse and unknown microbial colonisation on the paintings in
contrast to previous culture-dependant investigations.
In the past, the study of microbial communities and biogeochemical processes in hypogean environments is mainly related to the fact that microbes affect cultural heritage
properties that humans wish to protect (Groth & Saiz-Jimenez, 1999) and we owe much of our initial knowledge of cave microbiota to these studies. The role of actinomycetes in the
deterioration of paintings and frescoes in hypogean environments (not just caves, but crypts,
34 1.3 Microbial Biodiversity and Ecology of Caves tombs and underground churches) has been emphasised by many investigations (eg. Monte &
Ferrari, 1993; Groth & Saiz-Jimenez, 1999; Groth et al. 1999a). Actinomycetes are known to destroy wall paintings by the excretion of organic and inorganic metabolic products
(Schabereiter-Gurtner et al. 2004). The first actinomycetes identified as degraders of rock art were Streptomyces rectus fiexibilis, S. griseolus, S.cinereoruber, S.vinaceus, S.albus and Nocardia sp.
(Giacobini et al. 1988).
Though the role of actinomycetes in rock art is highly recognised, it is interesting that they haven't been isolated from works of art, except those located in hypogean environments
(eg. caves, crypts, grottos and tombs) (Giacobini et al. 1988). Atlanterra Shelter, Spain, contains rock art paintings made with iron oxides. The shelter is exposed to terrestrial environmental fluctuations. The bacteria isolated from Atlanterra Shelter seem to constitute a homogenous community with abundance of Bacillus strains, very different to actinomycete dominated communities found in rock art paintings from karstic hypogean environments (Groth & Saiz
Jimenez, 1999; Laiz et al. 1999; Gonzalez et al. 1999). All isolated Bacillus strains were able to reduce hematite which is significant due to the fact that Fe(ill)-(hydr)oxides are the most abundant pigments in rock art. This work demonstrates that actinomycetes are not alone in their role as biodeteriogens of rock art, however they do seem to be the dominant group in hypogean environments, perhaps indicating favourable selective pressures in the cave environment.
A number of actinomycetes isolated from caves have the ability to produce various types of crystals. Studies in Altamira and Tito Bustillo Caves demonstrate that the host-rock, cave formations and rock art are coated by dense networks of bacteria, mainly actinomycetes and these bacteria can induce constructive (calcification, crystalline precipitates) and destructive
(irregular etching, spiky calcite) fabrics. Because of this ability it has been proposed that these bacteria and others are directly or indirectly involved in constructive biomineralisation processes in caves (Laiz et al. 1999; Barton et al. 2001; Canaveras et al. 2001; Groth et al. 2001;
Jones, 2001). Little is known concerning the distribution, population dynamics, growth rates and biogeochemical processes of actinomycetes in caves, in spite of the fact that they seem to constitute a significant part of the "culturable" microbial population of these habitats. A
35 1.3 Microbial Biodiversity and Ecology of Caves prerequisite for the study of the role of actinomycetes in biogeochemical processes is the isolation and identification of these organisms (Groth et al. 1999a).
1.3.3.1 Actinobacteria
Stackebrandt et al. (1997) proposed a new hierarchic classification system, Actinobacteria classis nov. for the actinomycete line of descent, wholly defined by the phylogenetic analysis of small subunit 165 rRNA gene sequences. The Actinobacteria is comprised of high-G+C content
Gram-positive bacteria with a common ancestry and includes Subclasses Acidimicrobidae,
Rubrobacteridae, Coriobacteridae, Sphaerobacteridae and Actinobacteridae. The Order Actinomycetales
(actinomycetes) is within the Subclass Actinobacteridae. It is important to note here that quite often the actinomycetes are referred to simply as Actinobacteria, which, although fundamentally correct, is misleading, as the Class Actinobacteria encompasses a broader range of taxa than the
Actinomycetales alone. For the purpose of this study the term actinomycete(s) will be used to describe only members of the Class Actinobacteria, Subclass Actinobacteridae, Order
Actinomycetales.
1.3.3.2 Actinomycetes
Actinomycetes are Gram-positive bacteria which form branching hyphae at some stage of their development and may produce a spore bearing mycelium (McCarthy & Williams, 1990).
They are aerobic saprophytes and are widely distributed in nature (Goodfellow & Williams,
1983) mainly found in soil where they manufacture enzymes which degrade complex molecules and play a major role in decomposition of organic matter (Lechevalier & Lechevalier, 1985).
These organisms are selected for in environments characterised by oligotrophic conditions, low
water activities and high concentrations of CaC03. Hyphal actinomycetes are typically slow growing and their spores can remain viable for a number of years in unfavourable conditions; the exact length of time for which they can survive is uncertain. Although predominantly soil bacteria, actinomycetes have been isolated from a wide variety of environments, including
36 1.3 Microbial Biodiversity and Ecology of Caves freshwater, lake sediments, rivers, streams, marine environments, salt marshes, fodder and related materials, and air (Loyd, 1969; Cross, 1981; Hirsch & McCann-McCormick, 1985; Labeda
& Shearer, 1990). Actinomycetes have also been isolated from extreme environments such as; ice, sediments and air in Antarctica, and, as discussed previously, rock surfaces and sediments in cave environments (Eg. Cameron et al. 1976; Groth et al. 1999a,b).
1.3.3.3 Actinomycete Taxonomy
Over 150 genera of actinomycetes have been isolated from soils. The exact composition and phylogenetic boundaries of the actinomycetes has remained open to question and modification due to continued development and application of new taxonomic classifications.
Early attempts at taxonomic classification of actinomycetes were based on morphological and pigmentation characteristics of the sporing bodies and substrate mycelia, which is a useful but arbitrary approach to classification and not based on the phylogenetic relationships between different species (Williams et al. 1983). Variation in biochemical and physiological properties were incorporated into actinomycete taxonomy, however these new data alone could not be used to devise a satisfactory phylogenetically based taxonomy (Embley & Stackebrandt, 1994).
The rich chemical, morphological and physiological diversity of phylogenetically closely related genera of actinomycetes makes the description of families and higher taxa so broad that they become meaningless for the description of the enclosed taxa (Stackebrandt et al. 1997).
The application of molecular techniques based on variations in nucleic acid sequences between different bacteria, especially 165 rRNA gene sequencing, has had a dramatic impact on actinomycete systematics. It was soon discovered that some morphological characteristics given greater weight in earlier studies, such as the ability to form spores, were not reliable in a phylogenetic system of classification (Stackebrandt et al. 1981). Almost any description based on morphology or physiology would have exceptions and actinomycete taxonomy now relies heavily on molecular comparisons (Ensign, 1992). The only phenetic characteristics shared by all members of the actinomycetes is a relatively high level of guanine (G) and cytosine (C) as a
37 1.3 Microbial Biodiversity and Ecology of Caves percentage of total DNA (>55%) (Goodfellow, 1989). Actinomycete taxonomy is still under
development and more taxonomic information needs to be collected in all fields in order to
develop a phylogenetic system of classification with confidence (Holloway, 1997). To determine
a phylogenetic classification of actinomycete which is both true and practical it is necessary to
employ a polyphasic approach, employing a combination of molecular, chemical and numerical
taxonomic methods (Murray et al. 1990).
1.3.3.4 Actinomycete Ecology
As soil bacteria, actinomycetes contribute significantly to the turnover of complex
biopolymers, such as lignocellulose, hemicellulose, pectin, keratin and chitin (Williams et al.
1984). Additionally nitrogen-fixing actinomycetes of the genus Frankia have one of the broadest
host ranges known, forming root nodule symbioses in more than 200 species of flowering plants
(Huss-Danell et al. 1997). Actinomycetes can be recovered from most soils in relatively high
numbers although this may not give an accurate picture of proportions of active bacteria in the
soil because most of the colonies are probably isolated from spores (Williams, 1978). Streptomyces
and Arthrobacter are ubiquitous in soil and are the most numerous of the actinomycetes
(Goodfellow & Williams, 1983). The next most common actinomycetes are, in descending order,
members of the genera Micromonospora, Actinoplanes, Actinomadura, and Nocardia (Lechevalier &
Lechevalier, 1985).
Although soil is the main habitat of the actinomycetes, they can be isolated from
humans, animals, plants, waste water, food products, stones, buildings and works of art (eg.
Groth & Saiz-Jimenez, 1999). Despite intensive studies there are still many gaps in our
knowledge of the role played by actinomycetes in soil processes (Goodfellow & Williams, 1983).
Caves are unique environments characterised by little or no light, low levels of organic nutrients, and a stable, but cool to cold, microclimate. Russell, (1990), hypothesised that it is not
necessary for a microbe to function at optimal rates as long as it can compete effectively in its
38 1.3 Microbial Biodiversity and Ecology of Caves particular environment. It may be quite advantageous for cave bacteria to metabolise submaximally and have long generation times in nutrient poor environments.
Actinomycetes are well known for their ability to grow on nutrient poor media
(Lechevalier & Lechevalier, 1985) and streptomycetes can exist for extended periods of time as arthrospores that germinate in the occasional presence of nutrients (Goodfellow & Williams,
1983). Low temperatures are not a limiting factor for actinomycete growth. Suzuki et al. (1997) described an obligately psychrophilic actinomycete (Cryobacterium psychrophilum), and Xu et al.
(1996) reported actinomycete populations in cool areas of China, with average temperatures of
5° C or below 0° C, where Streptomyces spp. constituted up to 97% and 83%, respectively, of the total heterotrophic count. Some were psychrophiles with an optimum growth temperature of
10-15° C. Groth & Saiz-Jimenez (1999) suggested that growth of actinomycetes in hypogean environments might result from the association of two factors: low temperatures and high relative humidity. These environmental conditions, together with nutrient availability and nature of organic matter are recognised to be important factors controlling the activity of actinomycetes in caves.
39 1.4 Geomicrobiology
1.4 Geomicrobiology
Geomicrobiology is the term given to studies of the microbe-mineral interface, including microbial weathering and sedimentation processes, microbial roles in formation and degradation of minerals, mineralisation of organic matter, subsurface microbiology, biogeochemical cycling of elements, and bioremediation. Microorganisms are important active and passive promotors of redox reactions that influence geological formations (Ehrlich, 1999).
There is extensive literature demonstrating the influence of microorganisms in mineral formation from non-cave environments for a wide variety of minerals including, carbonates, oxides, phosphates, sulfides, and silicates (Fortin et al. 1997). Bacteria may produce minerals as a result of growth. Cell walls have chemically reactive sites that bind dissolved mineral-forming elements allowing nucleation and growth of crystals from an oversaturated solution to occur
(Groth et al. 2001). Alternatively, mineral precipitation may result from metabolic activities of bacteria. Bacterial activity may simply trigger a change in solution chemistry that leads to oversaturation and mineral precipitation. In biological processes, oversaturation is considered an important prerequisite for the precipitation of minerals from solution (Fortin et al. 1997).
Although Gonzalez-Munoz et al. (1996), suggested that this is merely incidental and the critical point is the participation of cellular membranes in inducing nucleation. Caves can be used as experimental study systems for geomicrobiology, not because they are strange, but because they are simple and often locally abundant, allowing for replicate studies (Northup & Lavoie, 2001).
While geomicrobiology in general has received substantial interest in the last decade, one unresolved issue is the involvement of microbial activity in the dissolution of, or formation of speleothems in caves (Barton et al. 2001).
1.4.1 Geomicrobiology in Caves
Caves are nutrient-limited environments containing a variety of redox interfaces and they provide an accessible window into subsurface environments in which to study precipitation and dissolution processes and products (Northup & Lavoie, 2001). A variety of 40 1.4 Geomicrobiology precipitation and dissolution processes results in the deposition of carbonate speleothems, silicates, iron and manganese oxides, sulfur compounds and nitrites and the break down of limestone walls resulting in corrosion residues. Geomicrobiological activities in caves are no longer underestimated since studies have shown that bacterial metabolism can affect these mineral precipitation and dissolution processes (Cai\.averas et al. 2001; Northup & Lavoie (2001).
Studies of microorganisms in caves have been predominantly descriptive, as illustrated in
Section 1.3, with only a few experimental studies reported although increased interest in microbe-mineral interactions in caves is emerging.
Microbially influenced corrosion or dissolution of mineral surfaces can occur through mechanical attack, the secretion of enzymes, and organic and mineral acids (eg. Sulfuric acid).
Microbially mediated reactions can generate considerable acidity that can dissolve cave walls and speleothems. Possible microbially influenced corrosion include limestone corrosion residues composed of iron and manganese oxides and clays (eg. Lechuguilla and Spider Caves, New
Mexico; Northup & Lavoie, 2001; Northup et al. 2003), and sulfuric acid speleogenesis and cave enlargement (eg. Movile Cave, Romania, and Cueva de Villa Luz, Mexico; Vlasceanu et al. 2000).
Microbially induced mineralisation is documented in the formation of carbonates, moonmilk, silicates, clays, iron and manganese oxides, sulfur, and saltpeter. For example, sulfate generated by sulfur I sulfide-oxidising bacteria can be used as an electron-acceptor by sulfate reducers. This reaction produces bicarbonate that can complex with calcium, resulting in the precipitation of calcite in the form of subaqueous mantles (eg. Weebubbie Cave, Nullabor, Australia) (Contos et al. 2001). There is no clear idea as to the significance of biological involvement in speleothem formation, however, there are clues.
Studies of cave geomicrobiology are largely still qualitative in nature. Barton et al. (2001) and Jones (2001) offered critical guidelines for the biogenicity of 'objects' visualised in cave deposits: they must, be found in a liveable environment, show complex form, show representations by numerous specimens, be members of a multicomponent assemblage, show morphological variability, reproduction by biological means, exhibit a range of degradation, organic residues and exhibit biogenic isotopic features. Various microbiological techniques have
41 1.4 Geomicrobiology been used to illustrate that microbes are present in most spelean environments and commonly modify the composition of the fluids and/ or influence precipitation of various minerals, including calcite (e.g. Melim et al. 2001). Classical isolation combined with molecular phylogenetic techniques reveals the presence of microbial communities associated with speleothems (Caiiaveras et al. 1999). Enrichment experiments with microorganisms cultured from cave environments have aided in identifying dissolution and precipitation abilities of these cave microbes (eg. Groth et al. 1999a) and stable isotope techniques has provided information on the microbial contribution to processes of mineral formation (eg. Hose et al. 2000) and ecosystem bioenergenetics (eg. Sarbu et al. 1996).
Most bacteria in nature live as part of dynamic metabolically interactive assemblages, commonly referred to as biofilms, found covering most solid substrates (rocks, plants, man made structures) (Douglas & Douglas, 2000). The primary techniques for examination of biological material on mineral surfaces are transmission electron microscopy (TEM), scanning electron microscopy (SEM), atomic force microscopy and environmental scanning microscopy
(ESEM) (Siering, 1998). Previous studies by Ray et al. (1997) and Douglas & Douglas, (2000) have shown the worth of ESEM for investigations of microbe-mineral relationships in natural microbial communities. Though SEM has been an important tool used to study cave microbial carbonates (Northup & Lavoie, 2001), ESEM allows the viewing of fully hydrated specimens that have not undergone structural or chemical alterations imposed by the extensive procedures necessary for viewing biological specimens in high vacuum necessary for conventional SEM.
Besides allowing visualisation of microorganisms in their natural form and as intact assemblages, ESEM also detects elements, especially those lighter that Si, which tend to be lost or masked by the processes used to prepare samples for conventional SEM (Douglas & Douglas,
2000).
The biogenicity of mineral-associated, purportedly biological features can be questionable and extremely difficult to resolve (Barton et al. 2001). Microbial activity has been directly or indirectly linked to the formation of many different minerals, however most geomicrobiology studies have focused their attention on the microbiological processes that are
42 1.4 Geomicrobiology associated with the development of carbonate deposits. Even with this focus, our knowledge of the microbial involvement in these processes has been limited by, i) the fact that there are few studies that have approached the issue from a geological perspective, ii) the fact that many geological studies of older deposits assume abiogenicity, iii) the fact that most geologists lack formal microbiological training, and iv) the scale of observation (Jones, 2001).
CaC03 speleothems predominate in most caves, and microbial studies have been conducted on stalactites, stalagmites, helictites, moonmilk, pool fingers and cave pearls.
Microorganisms have been found fossilised in carbonate speleothems (Jones & Motyka, 1987;
Polyak & Cokendolpher, 1992; Jones & Kahle, 1995; Melim et al. 2001). Fungi, algae and bacteria have all been implicated in the precipitation of carbonate dripstone in caves (Went, 1969;
Danielli & Edington, 1983). There is much evidence for rich and diverse chemoautotrophic and heterotrophic communities in caves (eg. Angert, et al. 1998; Sarbu, et al. 1996), it remains unclear however, what role, if any, these communities play in speleothem formation
1.4.2 Microbially Mediated CaC03 Precipitation
As some of the most abundant minerals on earth, carbonates are ubiquitous and highly reactive components of natural environments. Carbonate minerals play important parts in global carbon cycling, alkalinity generation, cycling of major and trace elements, and transfer of matter among oceans the continents and the atmosphere (Warren et al. 2001). Understanding carbonate precipitation has wide ranging implications from interpretation of biogeochemical
cycles, potential impact of increased atmospheric concentrations of C02 or reactive transport of radionuclides and trace metals in contaminated aquifers.
Bacterial precipitation of CaC03 has been reported in a variety of environments including hot springs, tidal mats and caves. It has been known since Boquet et al. (1973) that most
heterotrophic soil bacteria can induce CaC03 precipitation. Phillips & Self (1987) demonstrated that in soils with a high calcite concentration needle fibre-calcite formed within fungal mycelia and also encrusted rod-shaped microbes. Chafetz (1994) reported research carried out in the
43 1.4 Geomicrobiology field and laboratory conditions to demonstrate beyond doubt that CaC03 precipitation occurring within microbial mats was a process controlled by living bacteria and does not occur when the bacteria are dead, even in the presence of other living microorganisms.
Bacteria and fungi can precipitate CaC03 extracellularly through a variety of processes that include photosynthesis, ammonification, denitrification, sulfate reduction, and aerobic sulfide oxidation (Ehrlich, 1996; Castanier et al. 1999; Riding, 2000). Castanier et al. (1999)
proposed biologically mediated or active precipitation of CaC03 where carbonate particles are produced by ionic exchanges through the cell membrane of heterotrophic bacteria in an environment enriched in organic matter. Initially, this involves the adsorption of Ca2+ and
Mg2+ ions to negatively charged cell surfaces and the cell then acts as a nucleation site.
Subsequent CaC03 precipitation may be active or purely inorganic. Riding (2000) noted that microbial production of extracellular polymeric substances (EPS), which trap sediments, is often critical to the creation of microbial carbonates. Terrestrial oncoids (microbially formed carbonate constructions from dolestones, Cayman Islands) developed when calcifying filaments and spores trapped and bound detritus within the associated mucus (Jones, 1991). These resemble cave pearls, a speleothem that has been suggested to have a microbial association during formation (Gradzinski, 1997).
More recent studies have attempted to identify the factors that control the contribution of microorganisms to carbonate precipitation. Further progress in this field has been made in non-cave environments. Van Lith et al. (2003) found that only pure cultures of metabolising sulphate-reducing bacteria, isolated from hypersaline lagoons in Brazil, induced calcium dolomite and high magnesium-calcite precipitates indicating that the carbonate nucleation takes place in the locally changed microenvironment around the bacterial cells. Dittrich et al. (2004) showed that picocyanobacteria were involved in fast and effective calcite precipitation in an oligotrophic lake. Whether by saturation or nucleation they observed small calcite crystals produced by eukaryotic picoplankton whereas cyanobacterial picoplankton produced micritic carbonate indicating that different cells may induce very different, distinct precipitation processes.
44 1.4 Geomicrobiology As previously discussed, geological formations in caves (speleothems) like stalagmites and stalactites, are mineral depositions formed by precipitation of carbonates from ground water. Extensive documentation of microbial precipitation of CaC03 exists in non-cave literature, biogenic carbonates in particular have been studied since the late 19th century (eg. stromatolites; Chafetz & Buczynski, 1992). Microorganisms are believed to affect carbonate precipitation both through affecting local geochemical conditions and by serving as potential nucleation sites for mineral formation (McGenity & Sellwood, 1999). In natural environments, the primary means by which microorganisms promote CaC03 precipitation is by metabolic processes that increase alkalinity (Fujita et al. 2000). However, investigators have not established whether cave carbonate material has a similar origin.
Some of the most intriguing work on cave fungi associated with speleothem formation was conducted by Went (1969). The author made the interesting discovery that the growth of stalactites in Lehman Caves, Eastern Nevada, was associated with a fungus, Cephalosporium lainellaecola. This discovery was made using a special microscope mounted horizontally on an adjustable bracket sliding along a vertical steel bar so that stalactites could be observed in situ within the cave. He found that fungal hyphae occurred in a drop of water at the end of a straw stalactite and that strings of tiny calcite crystals tended to form along them. The hyphae not only functioned as crystallisation nuclei but also prevented the crystals from being removed with the falling drops. Perhaps actinomycete filaments act in the same way. Actinomycetes isolated from either dripping waters or rock in Altamira Cave showed the ability to produce crystals and therefore could play a role in the deposition of CaC03 polymorphs on the rock surface (Laiz et al.
1999). Although there is no known role for CaC03 in bacterial metabolism, certain organisms precipitate calcite during their growth (Buczynski & Chafetz, 1990). Groth et al. (2001), found that 45% of isolates from stalagmites in Grotta dei Cervi, Porto Badisco, Italy were able to precipitate CaC03 in culture medium. Organisms such as Achromatium oxaliferum contain internal calcite inclusions during growth (Head et al, 1996). There is also an established role for bacteria in the nucleation of CaC03 precipitation for stromatolite formation (Ehrlich 1999; Laval et al. 2000).
45 1.4 Geomicrobiology Various experiments have shown that bacteria may be replaced or encrusted by inorganic materials resulting in the fossil preservation of bacterial morphology. There are reports of bacteria preserved in carbonate rocks (Folk 1993; Jones 1995; Trewin & Knoll 1999) and a few reports of iron-oxidising bacteria preserved in carbonate speleothems in caves (Polyak
& Cokendolpher, 1992). However, although microfossils have been identified in carbonate speleothems, no direct connection with active precipitation processes in the formation of these features has been demonstrated. Bacterially induced changes in solution chemistry can be a passive process (eg. stromatolites; Chafetz & Buczynski, 1992). Evidence that microbes play a role in the formation of cave carbonates is still largely circumstantial and based on their physical presence. The question still remains whether the organisms identified are actively involved in speleothem formation, or simply buried during mineral precipitation (Polyak & Cokendolpher,
1992). Of special interest is the speleothem moonmilk. As discussed in Section 1.2.2, the wet pasty forms of moonmilk are so striking that some special explanation for their origin seems to be necessary. Caii.averas et al. (1999) suggested that bacteria present in caves may play a role in the formation of moonmilk deposits as microbial communities predominantly composed of different species of the genus Streptomyces were found in association with hydromagnesite and needle-fiber aragonite deposits in Altamira Cave.
1.4.3 Moonmilk
Moonmilk is a widely distributed, secondary formation and refers to the very hydrated white spongy /pasty or powdery masses found coating walls and speleothems in caves. It is not a mineral, it is a speleothem. It is often described as having a cottage cheese-like consistency and may be composed of several carbonate minerals. The historical term Mondmilch (=calcite moonmilk) is related to the proper type locality, the cave Mondmilchloch from South-Pilatus near Lucerne, Switzerland. Mondmilch was first mentioned by Agricola (1546, p. 194) and described by Gesner (1555) after visiting the cave Mondmilchloch (Fischer, 1988). This was without consideration of the actual mineral composition of the deposits. Moonmilk became well
46 1.4 Geomicrobiology known throughout Europe and used as a medication (Scheuchzer, 1752; in Fischer, 1988). In the
1 16 h and 11'1" centuries, physicians in Europe used dried moonmilk from caves as a dressing for wounds. Apparently moonmilk would stop the bleeding and act as a dehydrating agent.
However, some also believed it had curative properties. It is rather interesting that modem research or theories have discovered bacteria associated with moonmilk include actinomycetes that, as previously discussed, possess antibiotic properties.
Many descriptions of moonmilk are not only related to calcite growth, although the original term mondmilch from the cave Mondmilchloch refers to calcite precipitation and does not represent the phenomenon for speleothems in general. Hill & Forti (1986) suggested that texture rather than composition is implied by the term 'mondmilch'. Fischer (1988) defined mondmilch as a calcite microcrystalline or needle-crystalline speleothem with a minimum calcite content of 90 % weight, for the purpose of distinguishing true calcite mondmilch from other carbonate speleothems (< 90 % weight calcite) and other subterranean deposits, (eg. ferromanganese, sulfates, phosphates, silicates). The mineralogy and crystallography of potential mondmilch samples can be easily proved using X-Ray Diffraction Analysis (XRD) and scanning electron microscopy (SEM) methods (Fischer, 1988). Numerous synonyms in different languages exist for mondmilch, including the English version moonmilk.
True calcite moonmilk (mondmilch) has been found in many caves all over the world and appears to be particularly abundant in caves of cool temperature and high humidity. In warmer semi-arid regions limestones contain significant amounts of magnesium and moonmilk deposits may consist of a number of magnesium minerals including hydromagnesite, magnesite, huntite or dolomite (Moore & Nicholas, 1964). In Australian caves moonmilk has been documented in a variety of forms including, thin dry wall coatings, white cheese-like pasty forms at the bottom of rimstone pools or wall niche deposits, stalactites, cauliflower-like deposits and fluffy fungus-like forms in Jenolan Cave, NSW (http:/ /www.speleonics.com.au; maintained by J. Rowling). The origin of moonmilk deposits is highly contested among the literature. Hill & Forti (1986) cite four main theories as to the origin of moonmilk: i) freezing in ice caves, ii) precipitation from groundwater in which there is an agent which prevents the
47 1.4 Geomicrobiology crystals from growing large, (the theory preferred by Hill & Forti), iii) a disintegration product of bedrock, and iv) a by-product of the life cycle of various microorganisms. Each of these theories taken individually has its pros and cons as an explanation for the development of moonmilk.
White (1976) suggested that moonmilk in alpine caves may be precipitated chemically at low temperatures as hydrated carbonates, however these forms are only stable at low temperatures. Also freezing in alpine icy caves does not explain the occurrence of temperate and tropical moonmilk. Rapid precipitation of substances will generally result in small crystal size
and this occurs near cave entrances where precipitation is due to both outgassing C02 and evaporation of water (http:/ /www.speleonics.com.au; maintained by J. Rowling). It also occurs where gypsum is being produced. However, this does not explain the pasty textured moonmilk or that speleothems in cave entrances are hard and crystalline and quite unlike moonmilk.
Moonmilk is usually considered a depositional product. However, Hill & Forti (1986) suggested it can also form by corrosion processes. It is suggested that moonmilk could be a product of microbial metabolism which could biochemically corrode underlying bedrock. There are of course various types of bedrock and numerous disintegration processes that can occur within caves and though calcite deposits may be formed, they do not have the pasty texture that moonmilk is famous for. One common cause of bedrock disintegration is bat guano
(http:/ /www.speleonics.com.au; maintained by J. Rowling). It has been suggested that the thin films of moonmilk may be a result of bat guano bedrock disintegration, however this would not explain the moonmilk films in Entrance Cave, Tasmania, Australia, as there are no bats inhabiting Tasmanian caves due to cool air temperatures. Gradzinski et al. (1997) concluded that moonmilk deposits from several caves in Poland might be the result of microbial degradation of the host rock, as well as, or in place of microbially mediated precipitation of calcite. Conversely, in Spider Cave, New Mexico, SEM pictures of the microcrystals that make up moonmilk do not show the evidence of weathering that would be expected if microbial corrosion routinely resulted in moonmilk production (Northup & Lavoie, 2001).
48 1.4 Geomicrobiology It is generally accepted that moonmilk might be the by-product of the life-cycle of various microbes, although the question remains whether the organisms identified are actively involved or simply buried during mineral precipitation. A number of organisms have been
isolated from cave environments and shown to precipitate CaC03 in the laboratory (Danielli &
Edington, 1983; Groth et al. 2001). One very interesting point, a thick wall-niche deposit of moonmilk in Jenolan Cave is recorded as having been damaged by a person's handprint to at least 1 cm depth, yet 8 years later the print is/was no longer visible
(http:/ /www.speleonics.com.au; maintained by J. Rowling). Given the long length of time for usual speleothem growth (1 inch in 100-150 years; Section 1.2.2) this prompts the question as to whether the moonmilk was "alive" or not. Putative cells and an organic matrix can be frequently seen in moonmilk samples with SEM or in thin sections, but not in all cases. A wide range of microbes, particularly bacteria, streptomycetes but also fungi, algae and protozoa, can be cultured from moonmilk often in high densities (Northup et al. 2000).
Williams (1959) inoculated moonmilk samples from several caves in South Wales into various nutritional media and isolated eight species of heterotrophic bacteria belonging to the genera Bacillus, Micrococcus, Bacterium, and Streptomyces. In one culture a Gram-negative rod, a thiobacteria, was detected with the ability to produce CaC03 in crystalline forms similar to those found in moonmilk. Danielli & Edington (1983) isolated a wide range of colony types (mostly
Gram-negative cells) from moonmilk collected from caves in Wales and calcite precipitation was a common factor of these isolates. These authors suggested that cells were using the organic salt anion for energy and dumping the calcium as a waste product. When the calcium exceeded the solubility threshold, precipitation resulted. CaC03 encrusted cells then served as a nucleation site for further crystal formation. Gradzinski et al. (1997) proposed stages in the progressive formation of moonmilk where cells and an organic matrix first provide a structural framework; then, active bacterial cells are calcified and the extracellular organic matrix fills the remaining space with calcite. Although there is no known benefit of CaC03 precipitation in bacterial metabolism, detoxification of calcium has been suggested (Northup & Lavoie, 2001).
49 1.4 Geomicrobiology A very interesting cave phenomena usually associated with moonmilk deposits is the white/ grey silvered films which are covered in reflective dots and usually occur on walls and ceilings within the Twilight to Dark Zones of limestone caves and lava tube caves Gones, 1995)
Although there are no published works that this author could find, it seems to be widely accepted that the white/ grey coating is colonies of actinomycetes. The surface of these colonies is hydrophobic but the filamentous structures are hydrophilic and the droplets are attached to the end of these filaments. Lake & Rowling (pers. comm. J. Rowling, Aristocrat Technologies
Australia, 2004) collected some liquid from colonies at Jenolan Caves and investigated the mineral aspects of the liquid, and found that it was almost entirely calcite. These investigators postulated that perhaps these actinomycetes contributed to moonmilk deposits. The ability to form CaC03 polymorphs seems widely distributed among environmental actinomycetes; 19 out of 31 cave strains isolated and tested by Laiz et al. (1999) produced a considerable amounts of crystals in both solid and liquid media.
Microbial precipitation does not explain all forms of moonmilk. It is likely that there may be abiotic forms as well. An extensive survey of moonmilk deposits from high-altitude caves in the Italian Alps revealed no evidence of microbial involvement in calcite precipitation.
A review of factors contributing to the formation of moonmilk deposits in these alpine caves includes elevation and temperature, along with surface cover of soils and conifer forests and with low discharge rates of seepage water and high humidity (Borsato et al. 2000). However, the majority of samples were from fossil deposits (Borsato et al. 2000). Given the wide variability of minerals that may form moomilk it is not surprising that several mechanisms, biotic and abiotic, have been proposed for its formation, one or more of which may be involved in the deposition of moonmilk in a particular form or particular type of cave.
Biotic and abiotic hypotheses for the formation of moonmilk do not need to be mutually exclusive (Northup & Lavoie, 2001). Given the variety of mineral types involved and the range of physicochemical conditions, microbes are clearly involved in the formation of moonmilk by dissolution or by serving as nucleation sites in some cases, but they may play a minor or negligible role in other cases. Friedman & Sanders (1978) noted that "Purely inorganic chemical
50 1.4 Geomicrobiology reactions can take place only where simple organisms are totally absent. At the surface of the earth, environments devoid of such organisms are uncommon." That same observation is true for subsurface environments. Studies of dissolution and precipitation of carbonates, moonmilk, silicates, clays, iron and manganese oxides, sulfur, and saltpetre in caves span only a few decades. A variety of organisms with biogenic potential have been discovered and some fascinating systems and environments have been described from caves. These studies provide insights into biomineralisation in general, and in the formation of speleothems in particular
(Northup & Lavoie, 2001).
51 1.5 Significance
1.5 Significance
1.5.1 Biodiversity and Conservation Value
Biodiversity is the variety of all life forms: the different plants, animals and microorganisms, their genes and the ecosystems to which they belong. Australia is one of the most biologically diverse countries in the world with a large portion of its species found nowhere else in the world (1/5 of the world's diversity). Biodiversity underpins the processes that make life possible. Healthy ecosystems are necessary for maintaining and regulating atmospheric quality, climate, fresh water, marine productivity, soil formation, cycling of nutrients and waste disposal. Thus we depend on biodiversity for our survival and quality of life.
At the 1992 Earth Summit in Rio de Janeiro, world leaders agreed on a comprehensive strategy for "sustainable development", meeting our needs while ensuring that we leave a healthy and viable world for future generations (Department of Environment and Heritage,
Australian Biological Resources Study website; http:/ /www.deh.gov.au/biodiversity I abrs/).
One of the key agreements adopted at Rio was the Convention on Biological Diversity setting commitments to sustainable development. The two main goals established by the Convention were the conservation of biodiversity and the sustainable use of its components. The most significant impediment to the conservation and management of biodiversity is our lack of knowledge of it and the effects of human population and activities on it. Accordingly, a taxonomic perspective is necessary to conserve biodiversity and achieve sustainable development.
A taxonomic perspective includes providing underlying taxonomic knowledge of biodiversity and the environmental factors influencing species distribution in microhabitats.
Providing baseline information on the composition and distribution of cave microbial communities is essential to aid the conservation of cave microbial communities from human impacts.
52 1.5 Significance 1.5.2 Bioprospecting
A critical element in drug discovery based on microbial extracts is the isolation of
unexploited groups of microorganisms that are at the same time good producers of secondary metabolites. Together with their importance in soil ecology, actinomycetes are best known as a source of antibiotics. This became apparent in 1940, following Selman Waksman's seminal discovery of acti.nomycin (Waksman & Woodruff, 1940) and was fully realised by the 1980s when acti.nomycetes accounted for almost 70% of the world's naturally occurring antibiotics
(Okami & Hotta, 1988). Acti.nomycetes, represent an important source of biologically active compounds whose members have unparalleled ability to produce diverse secondary metabolites. These molecules present original and unexpected structure and are selective inhibitors of their molecular targets' (Donadio et al. 2002). Thus acti.nomycetes are a group of high economic, social and health significance.
In the past two decades there has been a decline in the discovery of new lead compounds from common soil-derived actinomycetes as culture extracts yield unacceptably high numbers of previously described metabolites (Mincer et al. 2002). Natural products continue to be a potent source of novel drugs and other bioactive compounds despite the
I emergence of combinatorial chemistry. The important attributes of natural products are their molecular diversity, still very much greater than that of combinatorial libraries, and their biological functionality (Nisbet & Moore, 1997). For this reason cultivation of rare or novel actinomycete taxa has become a major focus in the search for the next generation of pharmaceutical agents (Bull et al. 2000). The pharmaceutical industry has a strong interest in the acquisition of novel acti.nomycete biodiversity in the search for new lead compounds. There is strong incentive therefore to discover novel microbes whether it is done by exploiting molecular biology and/ or by exploring unusual biotopes (Colquhuon et al. 2000). Due to this interest significant biodiversity has been targeted and described from accessible environments. Williams et al. (1993) stated that one approach to the isolation of novel acti.nomycetes is to concentrate on understudied environments or substrates while using appropriate selective isolation techniques or to investigate habitats in which one or more of the environmental factors (eg. temperature,
53 1.5 Significance pH, aeration, or osmotic stress) are extreme. This has lead to the strategic targeting of extreme or unusual ecosystems. The importance of this area of rest:;arch has been recognised by the international research community, for example by recent EU funding of a new initiative at the
University of Newcastle upon Tyne ("New Approaches to the Discovery of Novel Bioactive
Compounds from Natural Actinomycete Communities").
Caves are unique ecosystems exposed to extreme environmental stresses. The limiting environmental characteristics of caves, little or no light, low levels of organic nutrients, high mineral concentrations and a stable microclimate, provide ecological niches for highly specialised and very diverse microbiota. Preliminary investigations of microbes isolated from the most remote and least human-impacted regions of Lechuguilla Cave, New Mexico, have highlighted their potential as sources of anti-cancer treatments, because of their ability to kill breast cancer cells (Northup & Mallory, 1998). Novel actinomycetes isolated from caves represent an important, potentially valuable biotechnological resource for the screening and discovery of novel bioactive compounds due to their origin from a unique and as yet poorly studied environment.
1.5.3 Bioremediation
Microbial biodiversity is a reservoir of resources that remains relatively untapped.
Microbes are the only life-forms that have been encountered in the deeper regions of the earths crust. Subsurface microbes with novel metabolic properties may be of potential value to industry for applications in bioremediation and biotechnology (eg. Gold, 1992; Boone et al. 1995;
Stevens & McKinley 1995; Bale et al. 1997; Krumholz et al. 1997, 1999; Chandler et al. 1998;
Whitman et al. 1998; Kieft et al. 1999; Takai & Horikoshi, 1999). In spite of recent findings, many of these microbial habitats remain poorly characterised mainly due to difficulties associated with access and sampling. Caves provide an accessible point of entry to the shallow subsurface.
Throughout.the world, organic and inorganic substances leach into the subsurface as a result of human activities and accidents, for example agricultural pesticides, landfill leachate.
54 1.5 Significance There, the chemicals pose direct or indirect threats to the environment and to increasingly scarce drinking water resources. At many contaminated sites the subsurface is able to attenuate pollutants that, potentially, lowers the costs of remediation. Natural attenuation comprises a wide range of processes of which the principle mediators are the microbiological component, which is responsible for intrinsic bioremediation, and can decrease the mass and toxicity of the contaminants by transforming or mineralising pollutants and is, therefore the most important
(Christensen et al. 2001; Roling & van Verseveld, 2002). Of particular relevance is the ability of subsurface microbes to induce formation of CaC03 minerals which presents an opportunity to develop and in situ bioremediation techniques for groundwater contaminated with divalent metals or radionuclides (Fujita et al. 2000). Reliance on intrinsic bioremediation requires methods to monitor the process. Knowledge of the subsurface geology and hydrology, microbial ecology and degradation processes can be used to monitor the potential and capacity for intrinsic bioremediation in the subsurface.
1.5.4 Biodeterioration & Biomzneralisation Processes
1.5.4.1 Palaeolithic Frescoes and Rock Art in Hypogean Environments
It is now well recognised that wall paintings can be severely damaged by microbial growth (Ciferri, 1999). It has been reported in the literature that pigment formation, crystal growth and other types of biodeterioration processes related to microbial activity affect rock paintings and frescoes in cave environments. In studies on the bacterial community associated with such deterioration, members of the actinomycetes both previously cultured and novel, are frequently cultivated (Sorlini et al. 1987; Weirich, 1989; Petushkova et al. 1990; Altenburger et al.
1996, 2002; Rolleke et al. 1996; Groth et al. 1999a; Wieser et al. 1999; Gurtner et al. 2000; Heyrman
& Swings, 2001; Gurtner et al. 2001; Heyrman et al. 2002). Studies in Altamira and Tito Bustillo
Caves, Spain, demonstrate that rock art paintings are coated by dense networks of bacteria, mainly actinomycetes. Identified damage includes: i) covering (scattered coloured spots, whitish powdery patinas, staining) of paintings by the microbial communities themselves and/ or by
55 1.5 Significance their metabolic activity (including biofilms and bio-induced precipitates); ii) chemical alteration, such as microbial mediated dissolution; and iii) mechanical alteration, such as rock substrate breakdown.
Bacteria can use organic compounds from the paint layer as growth substrates, producing acids, which cause discolouration of the paint or changes in its consistency. For example, iron-enriched pigments in rock art act as a substrate for attachment and a mineral supply for growth. In favourable conditions the bacteria present can change the colour of the paintings from the reddish yellow hues characteristic of iron pigments to a dark yellowish colour as a result of microbial metabolism. As noted previously in Section 1.4, some cave bacteria may play an important role in the precipitation and/ or deposition of CaC03 speleothems. Many of the actinomycetes isolated from caves are able to precipitate CaC03 crystals. These bacteria can induce constructive (calcification, crystalline precipitates) and destructive (irregular etching, spiky calcite) fabrics on the paintings and/ or surrounding rock.
Microbes can penetrate into the painting and its bedrock resulting in mechanical destruction of the cultural heritage (dissolution, etching of the host rock). In a study by Ca:fi.averas et al. (1999) a
Streptomyces xanthophaeus strain isolated from Tito Bustillo Cave walls was inoculated onto stalactite slices which showed pitting formation after only three months of culture in the laboratory illustrating a bacterially mediated calcite dissolution process. Because of this ability it has been proposed that these bacteria and others are directly or indirectly involved in constructive and destructive biomineralisation processes in caves (Laiz et al. 1999).
1.5.4.2 Monuments
Interestingly, a group of geomicrobiologists in Spain are following a unique view of biomineralisation processes by suggesting using bacterially induced carbonate mineralisation as a novel and environmentally friendly strategy for conservation of ornamental stone monuments.
Increasing environmental pollution in urban areas has been endangering the survival of
56 1.5 Significance carbonate stones in monuments and statuary for many decades. Numerous conservation
treahnents have been applied for the protection and consolidation of these works of art. Most of
them, however, either release dangerous gases during curing or show very little efficacy. There have been a number of studies looking at biomineralisation processes, particularly bio-mediated
calcite precipitation, for monumental stone conservation (Di Bonaventura et al. 1999; Tiano et al.
1999; Urzi et al. 1999), for example, Myxococcus xanthus -induced CaC03 precipitation efficiently
protects and consolidates porous ornamental limestone. (Rodriguez-Navarro et al. 2003). Calcite
precipitating cave isolates have the potential to contribute in this area.
1.5.5 Management Issues
Cave environments are generally quite stable. Diurnal changes have little effect on the
cave microclimate. Similarly, seasonal variations in temperature and humidity are relatively
minor. Air movement is regulated largely by cave morphology and if present, by the active watercourse. There are low numbers of macroscopic living organisms in caves, mostly insects
and spiders. In such a stable environment, microbial growth is the main threat to the preservation of the cave environment. The effects of microbial growth are exacerbated by human impact both on the external cave environment (eg. pollution, changed land use) and by visiting
the caves. Visitation produces a more direct and pronounced effect. Visitors produce variations in environmental conditions and increase microbial dispersal and colonisation, Humans can introduce foreign organisms from the surface environment that can establish in caves and they leave behind organic material (lint, hair, skin flakes etc) that provide a rich nutrient source for the proliferation of micro-organisms.
There are implications for Heritage Management in the case of hypogean environments containing Palaeolithic rock art. Pigment formation, crystal growth and other types of biodeterioration processes related to microbial activity affect rock paintings and frescoes in cave environments. These bacteria induce constructive effects such as calcification, crystalline
57 1.5 Significance precipitates, covering) and/ or destructive fabrics such as irregular etching, spiky calcite, substrate break-down and dissolution.
There are also implications for cave management issues include the impacts of changes in hydrology, cave sediment contamination on speleothems, and tourist cave lighting upon the natural microbial communities existing within cave microhabitats. Whether microbial communities are actively or passively involved in speleothem formation, disruptions to the natural communities will have an effect on the health and continued formation of speleothems and cave systems.
58 1.6 Conclusion
1.6 Conclusion
Cave environments represent one of few remaining isolated planetary habitats, in terms of human impact and the characterisation of novel microbial diversity. In the past, the study of microbial communities and biogeochemical processes in hypogean environments is mainly related to the fact that microbes affect cultural heritage properties that humans wish to protect and we owe much of our initial knowledge of cave microbiota to these studies. These studies may not necessarily reflect the biodiversity in 'natural' cave systems ie. those that are not heavily impacted by tourism. Compounding this, culture-based studies often have no 16S rRNA gene sequence data for isolates. Most published studies use morphological and biochemical means of identification, rather than phylogeny, to characterise cave strains to the genus level only. Thus it is difficult to make detailed comparisons at the species level between cave environments. Sequence data is available for described novel species from caves, however, little has been published about the cave environments that these novel species were isolated from.
It is widely accepted that only - 1 % of microbes are cultured in the laboratory. Culture independent methods are being increasingly used.to describe the composition of microbial communities and reveal significantly broader diversity than culture-based studies. Nevertheless, to date our knowledge of bacterial communities in caves is largely due to culture-based studies.
The past decade has seen a rapid increase in published investigations of microbial ecology in caves. However, the diverse range of types of caves (Eg. sulfur caves, carbonate caves, aquatic caves, tourist/show caves, restricted access caves) and microhabitats (Eg. acidic biofilms on walls, filamentous microbial mats in sulfur waters, aquatic microbial mantles, Palaeolithic rock art, cave walls, ferromanganese deposits, sediments) studied and the geographic separation of sites (Romania, Italy, Australia, Mexico, Spain, North America) makes it difficult to draw many comparisons or conclusions about cave microbial diversity (Eg. Sarbu et al. 1996; Angert et al.
1998; Vlasceanu et al. 2000; Holmes et al. 2001; Summers-Engel et al. 2001; Schabereiter-Gurtner et al. 2002, 2004; Northup et al. 2003; Chelius & Moore, 2004; Barton et al. 2004). Despite this recent expansion of our knowledge, literature on cave microbial communities, their distribution and
59 1.6 Conclusion taxonomic diversity, is limited and restricted to only a few caves world-wide, predominately in the northern hemisphere. In the southern hemisphere investigations of microbial diversity in caves is represented by only one publication. Holmes et al. (2001) investigated microbial diversity in unusual aquatic formations, mantles of mucus and biological material associated with crystalline material in submerged passages in the Nullabor Caves, Australia; a very unique microhabitat thus most likely not representative of general cave microbial biodiversity in the southern hemisphere. Molecular techniques are only recently being applied to geomicrobiological questions in hypogean environments (Eg. ferromanganese residues in
Lechuguilla Cave; Northup et al. 2003), and as yet there are no published culture-dependent reports of microbial communities associated with moonmilk deposits.
The description of the composition of microbial communities is an important starting point in studies of microbial biodiversity and sets the stage for fundamental studies concerning how these populations function (Morris et al. 2002). The microbial diversity of as yet poorly studied environments is being increasingly explored by molecular detection methods (eg.
Eppard et al. 1996; Rheims et al. 1996, 1998; Sarbu et al. 1996; Vlasceanu et al. 2000; Holmes et al.
2001; Summers-Engel et al. 2001; Schabereiter-Gurtner et al. 2002, 2004; Northup et al. 2003).
While molecular methods are valuable tools in characterising the microflora, isolation and culturing are still required for describing the microbial diversity, especially in the case of novel taxa (Palleroni, 1997).
60 Chapter 1: Introduction
SECTION 2:
MICROBIAL BIODIVERSITY IN TASMANIAN CAVES
Chapter 1: Introduction
Some of the deepest, longest and most beautiful caves in Australia are found in
Tasmania. Tasmanian caves are of mixed character (wet/muddy vs. dry) and range from commercially used caves to new or unexplored caves. Due to our southerly latitude, the caves in
Tasmania are colder and wetter than elsewhere in Australia with temperatures ranging as low as 4-7 °C. An interesting point to note is that there are no bats in Tasmanian caves, probably due to the cool air temperature in these caves. The Ida Bay Karst area is located in southern
Tasmania, mostly within the Tasmanian Wilderness World Heritage Area {Figure 1.1). Most of the karst retains native vegetation cover, which is wet sclerophyll forest and rainforest. The Ida
Bay Karst developed in Ordovician Gordon limestone from 510 to 439 million years ago (Mya), outcropping between 50 and 300 m above sea level. Cave development is substantial, with more than 140 cave entrances and in excess of 20 km of mapped passage, and predominantly CaC03 speleothems (Eberhard, 1999). The extensive cave systems in this region have a long and complex history of development, with Cainozoic (65 MYA to present) cold climate change exerting a major influence (Goede, 1968; Kiernan, 1982). Environmental conditions within the cave systems are thought to have changed little since they formed, except for periodic glacial sediment inclusion.
61 ....
Legend
Oual«n#y • Sikeout Sl'diment. OJallmlfY • Cek•eous Se
T«W-/·Sll~Sedirnenb Tet1art • Calc.eous Sediments Tertary·8as.al1 Crf:taceout • "'kallne lnt"usions
- Triffsit...kns5k-Basalt Trtasstc - CMbOnae:KttS Sedments C:J Pl"fmian-Triassk:·SiliceousSedment - SUo-()r(orUi • Sii~ 5edm«lts - ~Oevcrian · Slkerus Sediments - cambflen • Basalt m c.mo""'-"""" CWnliflan - SilkeousStdlrMnt'S CJ c.tnbNn • Felsic Volclrics [:::J Cam«!on-,,_ V_, c::J Cembrian- Ore Oeposits. !Ulran"'6G-M<1kcoml)le:•es1 Q c.ntirian - OreOtposits t Basall-gf*'fl'a<.ke~s l Neoprotero.r.oic· Basell mr1-"""'""·""""" Neopl"otemioic - Sedment Figure 1.1: Map of Tasmania depicting the World Heritage Area and Ida Bay karst region. Entrance-Exit Cave system and Loons Cave are located in the Ida Bay karst. Overlay detailing geology of Tasmania, including calcerous sediments of the Ida Bay karst region. Data provided by National Parks and Wildlife Service Tasmania. ou.wn..;- ewtS~ ~- Clllc•.aus~ o~- iO.t#llll P"91a11fHUff CJ"'-"">·""*'-"'-- lfftary- Sllcw.n ~ T~-Catc..wt~ r...., . ~,,,,. 0-elaCAOul - Nkllllne "*usionl ..WM - ~ - T~ff• • BH"'1 ~ . c.banac9CU5 s.canents Q Plfmian-Tt1Mlic . Siiiceous s.dnteots c::J P«miM'I • Calc•eout S9dlmtnb OtYonlan . Ol'...W. - SUo-~ - Sllcews S9dlrMntl _.'aliai.-ili' llil>W~ ~ 'Ht!ritage Area - ~-"""""'C.ntirian -Sltbo1ot1~ . Ida Bay karst: Entrance-Exit Cave Loons Cave 62 Chapter 1: Introduction Figure 1.1: Map of Tasmania depicting the World Heritage Area and Ida Bay karst region. Entrance-Exit Cave system and Loons Cave are located in the Ida Bay karst. Overlay detailing geology of Tasmania, including calcerous sediments of the Ida Bay karst region. Data provided by National Parks and Wildlife Service Tasmania. Ida Bay karst: Entrance-Exit Cave Loons Cave 62 Chapter 1: Introduction The biological importance of the Ida Bay caves has been recognised for more than 100 years, beginning with an article published in Scientific American describing the spectacular glow worm display in Entrance Cave (Anon. 1895 in Eberhard, 1999). Over the years, many rare and endemic obligate cave fauna have been discovered and described from Ida Bay caves resulting in this region being widely recognised as containing one of the more diverse and significant assemblages of cave fauna in Australia's temperate zone (Richards & Oilier, 1976). The Entrance-Exit Cave System is a site of high biological significance, the most outstanding biological feature of the caves being the glow worm display. The Entrance Cave subsystem, in particular, is the type locality for many obligate cave dwelling fauna (Richards & Oilier, 1976). Near the entrance and extending for some distance into Entrance Cave there is a very significant cave fill deposit consisting of a conglomerate of rounded boulders and pebbles set in a fine matrix and thoroughly indurated. This deposit has not been studied in detail but an intelligent guess is that it is sediment of glacial times, when solifluction was prevalent but running water was much reduced (Richards & Oilier, 1976). The significant feature is that this , deposit extends to roof level which possibly means it blocked the cave completely at one stage allowing 'evolution' in isolation and has since been largely removed by subsequent stream action (Richards & Oilier, 1976). Loons Cave, although very dose in proximity, is a very different system to the Entrance Exit Cave System. Loons Cave essentially consists of a single, narrow, low energy stream passage that appears to be fed primarily by waters of seepage origin not a streamway originating from the surface (Household & Spate, 1990). The cave is reasonably well decorated with speleothems that are generally massive and robust. Loons Cave is commonly used as an "outdoor experience" locality for school and recreational groups and is therefore a site of high human impact in contrast to the majority of the Entrance - Exit Cave system. Deposits of moonmilk are a common feature of many Tasmanian caves (Goede, 1988). Despite their abundance they are amongst the least studied and understood of any of the cave 63 Chapter 1: Introduction deposits. Very large moonmilk deposits are evident in Exit Cave occurring as a uniform or botryoidal layer that covers stalactites, cave walls, ceilings and floors. Entrance Cave is also known to have moonmilk deposits although on a much smaller scale than Exit Cave. Within the Entrance Chamber of Entrance Cave, just beyond the cave mouth, large white mats with silvered droplets (similar to those described in Section 1.4.3) are visible on the ceiling rock. These have been anecdotally described as being actinomycete colonies by enthusiastic cavers, though this has previously not been investigated. The white mats are visible past the Twilight Zone of the cave and in the Dark Zone, however not to the same extent. Although there are no moonmilk speleothems in Entrance Cave per se, it was discovered during the course of this study that there are large deposits of moonmilk beneath the sediment throughout the cave. The focus of this research was the characterisation of microbial biodiversity from Tasmanian caves (Entrance-Exit Cave system and Loons Cave) in 3 microhabitats; sediments, speleothems and moonmilk deposits. Isolation of pure cultures reveals only a minor fraction (- 1 %) of the actual biodiversity in an environment. Culture-independent 16S rRNA gene sequence analyses have opened the way to study bacterial communities in environmental samples without prior cultivation and reveal a significantly broader diversity than culture-based studies (Amann et al. 1995; Head et al. 1998; Hugenholtz et al. 1998). Bacterial diversity in Tasmanian caves have not been investigated using culture-independent techniques and to date there is no published culture-independent study on moonmilk worldwide. Thus classical isolation and molecular detection methods (DGGE, 16S rRNA gene clone library analysis) were used to compare culturable vs. non-culturable biodiversity, particularly of the actinomycetes who appear to dominate isolations from culture-based studies of heterotrophic cave systems. To expand our knowledge of cave microbial diversity, phylogenetic analysis was used to determine diversity at the species level and to infer ecological function where possible. The biodiversity described acts as a baseline for assessing environmental impacts and also identifying factors influencing microbial diversity. 64 Chapter 2: Materials and Methods Chapter 2: Materials and Methods 2.1 Site description and sample collection 2.1.1 Entrance-Exit Cave System The Entrance Cave subsystem has a simple cave opening where Mystery Creek goes underground and is located approximately 2 km from Ida Bay, along the South Lune Road. The cave follows the course of Mystery Creek entering the north side of Marble Hill, also known as Caves Hill, at an elevation of 115 m (Richards and Oilier, 1976). The cave floor is a riverbed, covered with large boulders and cobbles. Water and nutrients are contributed to the lower level passages by the active inflow stream Mystery Creek, whereas the upper level passages are dry. Mystery Creek re-emerges via a non-negotiable route into Exit Cave and a subterranean section of the D'Entrecasteaux River draining out of the south side of Marble Hill. Exit Cave is the longest cave in Australia with greater than 15 km of passages, generally large sized. Mystery Creek is also an important inflow stream to the Exit Cave subsystem, contributing water and nutrients. There are also many smaller feeder passages in the Exit Cave subsystem with low energy streams and more than 100 other known caves in the Ida Bay karst that are predominantly vertical shaft caves on the slopes of Marble Hill and connect with the Exit Cave subsystem at depth. 2.1.2 Loons Cave Loons Cave essentially consists of a single, narrow, low energy stream passage that appears to be fed primarily by waters of seepage origin (Household & Spate, 1990). The natural, undisturbed substrate in this stream consists of a lightly cemented veneer of pebbles overlying a deep unconsolidated mass of fine clay sediment. The effect of repeated trampling on this sensitive veneer has caused its breakage and collapse into the underlying soft sediments, 65 Chapter 2: Materials and Methods resulting in the formation of deep muddy pools. Parts of the stream substrate remain in original, pristine condition where it crosses underneath sections of passage inaccessible to people. 2.1.3 Sample Collection Samples were collected from Entrance, Exit and Loons caves, concentrating on three microhabitats; floor sediments, speleothems and moonmilk deposits. Sites were chosen with minimal contamination factors and to reduce impact of our sampling to a minimum. Samples were collected to the side of the main paths to avoid contamination from trampling of cavers and 'clean' speleothems and moonmilk were chosen with no visible human impact or handling (e.g. mud smears, hand prints etc.). Samples were collected under the provisions of permit number ES 01147 issued by National Parks and Wildlife Service, Tasmania. Sediment sampling consisted of collecting approximately 10 g/sample using a sterile teaspoon and placing into individual sterile plastic bags. Sterile swabs (EUROTUBO® Collection Swabs; I.A.S.A) moistened with sterile double distilled water (ddHP) were used to sample from spel~othems. To collect moonmilk deposits, MEl and 3, in Entrance Cave, the upper layer of sediment was scraped away with a sterile teaspoon and sterile 15 mL falcon tubes (REDLINE Scientific Pty. Ltd.) were inserted into the deposit. The tubes were withdrawn from the deposit approximately half full and capped immediately. Similarly, samples were collected from moonmilk speleothems in Exit Cave, MXl, by inserting sterile 15 mL falcon tubes into the formation till they hit the 'hard' speleothem surface, withdrawing and capping immediately. Samples of the white mat, ME2, in Entrance Cave were collected by inserting glass slides between the mat and mud or substrate rock. The slides were placed on wet tissue paper within closed petri dishes to keep them hydrated. Samples were transported to the laboratory on ice and stored at 4 °C until processed. Sample locations and descriptions are listed in Table 2.1. 66 Table 2.1: Identity, location and description of samples collected from Entrance, Exit and Loons Caves Sample* Cave and sample location Descnption SEl Entrance Cave, Big Stalagmite Cavern; Dark Zone Dry sediment from indentation, 1.2 ms above floor, Big StalStalagmite. SE2 '"' Wet sediment from front drainage region of flow form by Big Stalagmite SLl Loons Cave, "Tarpit", Dark Zone Dry sediment from left hand sidewall deposit above flood zone. SL2 1111 Wet sediment from bottom of 1 m deep permanent mudhole. SPE3 Entrance, Big Stalagmite; Dark Zone Swab, droplet on shelf roof, nght hand side of passage. SPES un Swab, wet flow form, right corner of passage entry. SPE7 un Swab, Big Stalagmite, dry surface, 1.5 m above floor. SPElO Entrance, Big Flow form; Twilight Zone Swab, moonmilk mat on cave roof. SPE12 Entrance, left hand platform; Twilight Zone Swab, old dry flow form. SPL2 Loons, First Aven; Dark Zone Swab, large dnp stone under aven. Swab, red droplet on fungal mycelia. SPL3 Loons, dry platform past first Aven; Dark Zone n SPL6 Loons, Lower entrance crawl; Twilight Zone Swab, sloping surface among small stalagmites. g" SPL8 Loons, Sump; Dark Zone Swab, cream flowstone surface. (b" 1-j SPL9 1111 Swab, carrot stalactite. ~ 1111 ~ SPL12 Swab, cream flowstone pools. PJ (b" MEl Entrance Cave, Cave Mouth; Light Zone Moonmilk beneath sediment of boulder 1-j...... ,_.PJ ME2 Entrance Cave, Entrance Chamber; Twilight Zone White mat on ceiling mud and rock rJl PJ ME3 Entrance Cave, Second Chamber; Dark Zone Moonm1lk beneath sediment cave floor g, MXl Exit Cave, Ballroom Chamber; Dark Zone Stalactite with thick coating of moonmilk ~ rog 0\ *Samples catalogued using the following code: the first character(s) represent the m1crohabitat (S =sediment, SP = speleothem, M = moonmilk), the last p... '-.:i character represents the cave (E =Entrance, X =Exit, L =Loons). Number 1s indicative of the site that samples were collected from. All samples collected rJl by Jodie van de Kamp and Dr David Nichols, with base support from Dr. Kevin Sanderson during 2001 and 2002 Permit number ES 01147 issued by National Parks and Wildlife Service, Tasmania. Chapter 2: Materials and Methods 2.2 Microscopy and Mineralogy 2.2.1 ESEM and X-Ray Elemental Microanalysis ESEM was used to visualise microbes within the moonmilk matrix. Fresh, unfixed samples were viewed by ESEM approximately 4 h after collection. Small pieces of moonmilk were removed from the glass slides or falcon tubes using a sterile scalpel blade and placed on aluminium SEM stubs for viewing by ESEM 2020 (Phillips, Australia). The elemental composition of specimens was obtained by means of X-Ray Microanalysis (pers. comm. David Steele, University of Tasmania, 2002). 2.2.2 X-Ray Diffraction Analysis Mineralogical compositions of moonmilk were determined by X-Ray Diffraction (XRD) Analysis. Moonmilk samples were prepared by drying, grinding to <-10-75 µm and pressing into a 25 mm diameter aluminium sample holder. The samples were run on an automated Philips X-Ray Diffractometer system: PW 1729 generator, PW 1050 goniometer, PW 1710 microprocessor, with nickel-filtered copper radiation at 40 kV /30 mA, a graphite PW 1752 monochromator, sample spinner and a PW 1711 sealed gas filled proportional detector. The PW 1710 system is driven by software packages, "Visual XRD v 2.6" (Diffraction Technology, Australia) and "PW 1710 for Windows" (CSIRO, Australia), with plotting software, "XPLOT for Windows" (CSIRO, Australia) and "Traces v 5.1" (Diffraction Technology, Australia). Interpretation was mostly by manual methods. Samples were calibrated with an internal standard of natural quartz. The semi-quantitative mineralogy was determined by manual search-match methods using a series of prepared standards (pers. comm. Ralph Bottril, Mineral Resources Tasmania, 2003). 68 Chapter 2: Materials and Methods 2.3 Isolation and Identification of Microbes 2.3.1 Isolation and culturing of microbes Microbes were isolated from sediments using selective isolation procedures developed by the Antarctic Microbiology Group (University of Tasmania). Approximately 5 g of sediment was transferred into a sterile petri dish and left open in a laminar flow (Gelman Sciences, Australia) overnight to dry. Sediments were ground to an even consistency using a sterile mortar and pestle and then divided into two equal portions by weight; one untreated control sample (overnight drying and incubation at room temperature for 2 h; OD) and one treated sample (overnight drying and subjected to a heat treatment of 70 °C for 2 h; ODM. Samples were transferred to individual McCartney bottles containing 9 mL of sterile dd H 20 and placed on a tube roller (Luckham Ltd.) for 30 min to mix. Microbes were isolated from moonmilk using a modified version of an isolation procedure developed by Olivier Braissant (pers. comm. Universite de Neuchatel, Germany, 2002). Similarly to sediments, up to 5 g of moonmilk (moonmilk being very light in comparison to sediments) was weighed into petri dishes, dried overnight, ground, and divided into four equal portions by weight. Samples were subjected to one of four different treatments by transferring to individual McCartney bottles containing either: 1) 5% acetic acid (CH3COOH) in 0.01 M MgS04.7HzO; 2) 1% acetic acid in O.OlM MgS04.7H20; 3) 1 mM Ethylenediaminetetraacetic Acid (EDTA); or 4) 0.1 mM EDTA. Samples were then placed on a tube roller for 30 min to mix. Dilution series to 10·3 were prepared for sediment and moonmilk samples (initial bottle 10°) and 0.1 mL of each dilution spread plated in duplicate on selective media that favours the growth of actinomycetes; Starch-Casein Agar (SC) (Kuster & Williams, 1964), Arginine-Vitamin Agar (AV) (Nonomura & Ohara, 1969), Marine Agar (MA) (Oxoid 2216) and R2A Agar (R2A) (Oxoid CM 906) and non-selective agar for moonmilk samples only; 1/2 strength Tryptone Soya Agar (1/2 TSA) (Oxoid CM 129) (see Appendix 1 for culture media recipes and preparation). Swab samples were directly streaked onto the above selective media immediately on return 69 Chapter 2: Materials and Methods from sampling trips. Plates were left to dry in a laminar flow for 30 min. Plates were sealed with 0 2 permeable parafilm (American National Can™, USA) and duplicates .incubated at 25 °C (within optimal temperature range for isolation of actinomycete) and 10 °C (representing the cave environment) for 2-4 wk or until there was sufficient growth of colonies. After .incubation, actinomycete-like colonies were selected from the primary plates and sub-cultured on Oatmeal Agar (OA) (Williams & Wellington, 1982) (see Appendix 1). For moonmilk samples, non actinomycete-like colonies were also selected and subcultured on 1/2 TSA. Secondary plates were .incubated at 25 °C for approx. 1 wk. All further sub-culturing was conducted as described until pure isolates were obtained. Isolates were cryopreserved (see Appendix 2 for protocol) in replicate for long-term preservation and future use. 2.3.2 165 rRNA gene sequencing and phylogenetic analysis of isolates 2.3.2.1 Extraction of nucleic acids and purification Genomic DNA was extracted using a method modified from Marmur (1961). Culture biomass was harvested by scraping with a sterile loop. Cells were resuspended in sterile 1.5 mL microcentrifuge tubes (Eppendorf; Greiner Bio-one) with 400 µL saline-EDTA (pH 8) and 1 vortexed (MT 17 Vortex; CHILTERN) to mix. 50 µL of lysozyme (40 mg mL- ; AMRESCO) was added and the tubes .incubated for 30 m.in at 55 °C in a M20 waterbath (LAUDA). 20 µL of 1 proteinase K (10 mg mL· ; SIGMA) was added and the tubes again .incubated for 15 m.in at 55 °C and 20 µL of 25% (w /v) sodium dodecylsulphate (SDS) (SIGMA) for a further 30 m.in at 55 °C. Tubes were mixed by vortexing between each incubation step. Samples were then subjected to a freeze/thaw step by incubation at-20 °C overnight and thawing at 55 °C for 30 min. Cell debris was separated from aqueous DNA solution by centrifugation at 14000 rpm x 5 m.in, 4 °C in a bench top Eppendorf Centrifuge 5417 R (Laboratory Supply Australia Pty. Ltd.). The supernatant (approx. 400 µL) was transferred to a new sterile microcentrifuge tube. DNA was extracted twice by adding an equal volume of 25:1 (vol/vol) chloroform-isoamyl alcohol 70 Chapter 2: Materials and Methods {SIGMA), followed by vortexing and centrifugation at 14000 rpm x 10 min, 4 °C. The aqueous phase was transferred to a new, sterile microcentrifuge tube each time. DNA was further purified using the Prep-a-Gene® DNA Purification Kit (Bio-Rad) reagents and protocol. DNA products were stored at -20 °C. 2.3.2.2 Agarose gel electrophoresis To analyse extracted nucleic acids they were fractionated by electrophoresis through 1.0- 1.5% (w /v) agarose (AMRESCO) gels with 0.5 µg/mL ethidium bromide (EtBr) in Tris-acetate EDTA buffer (40 mM Tris-acetate; 1 mM disodium EDTA; pH 8) {TAE), in a mini-gel apparatus (Horizon 58, Horizontal Gel Electrophoresis, BRL). 5 µL of DNA product was mixed with 3 µL of 6x gel loading buffer (0.25% bromophenol blue; 0.25% xylene cyanol FF; 40% sucrose) and loaded into the gel. To determine the size of nucleic acid fragments, samples were run alongside 5 µL of the DNA molecular weight marker HyperLadder I (Bioline). Electrophoresis was carried out using a Power Pack 300 power supply (Bio-Rad) at 80 V for 30 min. The DNA/EtBr complex was visualised under short wavelength ultra-violet radiation on an electronic ultraviolet light transilluminator (Ultra. Lum. Inc.). 2.3.2.3 Determination of DNA concentration The concentration of DNA and PCR solutions (DNAconc) was determined by measuring absorbance at 260 nm using a spectrophotometer (Pharmica) and calculated using the following equation: 1 1 1 1 DNAconc (mg mL- = µg µL- ) = (A260 x 50 µg mL- x D) / 1000 µg mL- Where D = dilution factor 71 Chapter 2: Materials and Methods 2.3.2.2 165 rRNA gene PCR amplification and purification The 165 rRNA gene fragment was amplified by Polymerase Chain Reaction (PCR) from extracted genomic nucleic acids using two universal primers, 10 forward and 1500 reverse (5tackebrandt et al. 1991) (Table 2.2). These primers were used as they gave thorough coverage of the three hypervariable regions in the 165 rRNA gene fragment (5tackebrandt et al. 1991). PCR was performed using the Hot5tarTaq™ PCR Master Mix Kit (QlAGEN) reagents and protocol. PCR reactions consisted of: Hot5tarTaq Master Mix 25µL Primer 5' (50 pmol) 2µL Primer 3' (50 pmol) 2µL Q-5olution* 2.5 µL Template DNN' __l__g1 ddH20 to total volume 50 µL * Q-Solution changes the melting behaviour of DNA and was used for PCR reactions that did not work well under standard conditions. A Amount of template DNA added to PCR mix varied depending on the concentration of the DNA, however in most cases 2 µL was sufficient. PCR reactions were carried out in a PTC - 200 Peltier Thermal Cycler (MJ Research) using the following parameters: Initial activation step: 15min 95 °C 3-step cycling: Denaturation: lmin 94°C Annealing: lmin 52 °C Extension: 3min 72 °C Number of cycles: 30 Final extension: lOmin 72 °C* *The final extension step is prolonged to 10 min to allow full extension of any partly amplified DNA fractions. PCR fragments were purified using the Prep-a-Gene® DNA Purification Kit (Bio-Rad) reagents and protocol. PCR products were electrophoresed as described previously to ensure fragments of the correct size were obtained, and to determine quantity and quality. PCR products were stored at -20 °C. 72 Chapter 2: Materials and Methods 2.3.2.3 165 rRNA gene sequencing PCR products were sequenced directly using the CEQ 2000 Dye Terminator Cycle Sequencing (DTSC) Quick Start Kit (Beckman Coulter) reagents and modified protocol. For initial identification of microbes universal primer 519 forward (Stackebrandt et al. 1991) (Table 2.2) was used for amplification. To obtain full sequence information of selected isolates, universal primers 10 forward and 1500 reverse were also used. Sequence reactions consisted of: DTCS Quick Start Master Mix 2µL Primer (5 pmol) 1 µL Template PCR* XµL ddHzO to total volume 10 µL *According to Template Preparation Table in CEQ 2000 DTSC protocol. Amplification parameters were: Denaturation: 96 °C 20 sec Annealing: 50 °C 20 sec Extension: 60 °C 4min Number of cycles: 35 Amplification reactions were purified by ethanol (EtOH) precipitation according to the CEQ 2000 DTCS protocol. Subsequent electrophoresis and analysis was performed using an automated CEQ™ 2000XL Genetic Analysis System (Beckman Coulter). In most cases, 16S rRNA gene fragment sequences spanned nucleotide positions 519-1540 (E.coli equivalent). Entire 16S rRNA gene sequences spanning nucleotide positions 10-1540 were obtained for novel isolates. 73 Chapter 2: Materials and Methods Table 2.2: Primers used for PCR amplification and sequencmg of 165 rRNA gene fragments. Pruner Bindmg Primer Sequence (5' to 3') (Reference) Region• 10 (f) 10-29 GAG TIT GAT CCT GGC TCA G (Stackebrandt et al. 1991). 1500 (r) 1520-1540 AGA AAG GAG GTG ATC CAG CC (Stackebrandt et al. 1991). 519 (f) 519-536 CAG CMG CCG CGG TAA TAC (Stackebrandt et al. 1991). 1392 (r) with GC clamp 1406-1392 CGC CCG CCG CGC CCC GCG CCC GGC CCG CCG CCC CCG (Ferris et al. 1996) CCC CAC GGG CGG TGT GTA C 907 (f) 907-926 GGC AGT TAA GGA AAC TCA AA (Santegoeds et al. 1998) pUCIM13 (f) NIA GTA AAA CGA CGG CCA GT (Promega) pUCIM13 (r) NIA CAG GAA ACA GCT ATG AC (Promega) •Number is based on the Escher1chia coli numbering system from Brosius et al. 1981 2.3.2.4 Phylogenetic Analysis Sequence electrophoretograms were examined using the program CHROMAS (http: I /www.technelysium.com.au/chromas.html) in order to resolve any ambiguous base positions. 16S rRNA gene sequences were initially analysed using the National Center for Biotechnology Information (NCBI) database, Genbank, BLAST tool (http://www.ncbi.nlm.nih.gov/blast/blast.cgi; Altschul et al. 1997) to identify related sequences available in public databases and to determine phylogenetic groupings of sequences. For phylogenetic analysis, sequences were aligned using the program BioEdit (http://www.mbio.ncsu.edu/BioEdit/bioedit.html; Hall, 2001) for comparison with validly described and published sequences of representative members of the actinomycete obtained from NCBI GenBank. Distance matrices and phylogenetic dendrograms using the neighbour- joining method were generated using programs DNADIST and NEIGHBOUR of the PHYLIP 3.573c package (Felsenstein, 1993). 74 '' ., Chapter 2: Materials and Methods 2.4 Molecular Analysis of Sediments and Moonmilk 2.4.1 Extraction and purification of nucleic acids from environmental samples 2.4.1.1 Sediments Total nucleic acids was extracted from sediment following a method modified from Purdy et al. (1996). Approximately 0.5 g of sediment was aseptically transferred to a 2 mL screw cap microcentrifuge tube (Astral Scientific) containing 0.5 g of 0.1 mm diameter zirconia-silica beads (Biospec Products) and suspended in 700 µL 120 mM sodium phosphate buffer (pH 8.0) (Na2HP04), 500 µL Tris-equilibrated phenol (pH 8.0) (AMRESCO), 50 µL 20% (w /v) SDS and 1 % acid-washed polyvinyl-polypyrrolidone (PVP) (AMRESCO). To lyse the soil microbes, the sample was disrupted in a mini-beadbeater (Biospec Products) at 3 800 rpm for 3 x 30 sec pulses, with a 30 sec incubation on ice between pulses. Cell debris was separated from aqueous DNA solution by centrifugation at 12000 rpm x 2 min, 4 °C. The supernatant was transferred to a new sterile microcentrifuge tube and incubated on ice. The pellet was resuspended in 700 µL 120 mM Na2HP04 Buffer (pH 8.0) to extract residual nucleic acids from the sample. Cell disruption and centrifugation was repeated as described and the supernatant removed and pooled with the first extraction. Nucleic acids were precipitated by adding 0.1 volumes of 3M sodium acetate (pH 4.6) (NaOAc) and 2 volumes of cold absolute EtOH followed by incubation at -20 °C for at least 30 min, preferably overnight. The supernatant was removed after centrifugation at 14 OOO rpm x 30 min, 4 °C. The DNA pellet was washed twice in 3~0 µL cold 70% EtOH, with further centrifugation at 14 OOO rpm x 5 min, 4 °C. After removing the supernatant the pellet was allowed to air dry in a laminar flow hood and subsequently resuspended in 40 µL sterile ddH20. 2.4.1.2 Moonmilk Nucleic acids were extracted by a procedure developed for this study, modified from Miller et al. (1999); the Phosphate, SDS, Chloroform-Bead Beater method (PSC-B) (pers. comm. Susan Turner, University of Auckland, New Zealand, 2003). Approximately 0.5 g of moonmilk was aseptically transferred to a 2 mL screw-cap microcentrifuge tube containing 0.5 g of 0.1 mm 75 Chapter 2: Materials and Methods diameter zirconia-silica beads (Biospec Products) and 300 µL 100 mM Na2HP04 (pH 8.0) and 1 resuspended by vortexing. 30 µL lysozyme (50 mg mL- ) was added and the tubes incubated at 37 °C for 30 min, followed by a further incubation at 65 °C for 60 min to enhance lysis of the cells. Following incubation, 300 µL of SDS lysis buffer (100 mM NaCl, 500 mM Tris pH8, 10% SDS) was added and the tubes inverted to mix, followed by adding 300 µL chloroform-isoamyl alcohol (24:1; v /v) (SIGMA). Samples were mechanically lysed by bead-beating at 4 OOO rpm for 2 x 40 sec pulses, with a 40 sec incubation on ice between pulses. Cell debris was pelleted from aqueous DNA solution by centrifugation at 12000 rpm x 5 min, 4 °C. The supernatant, approximately 650 µL, was transferred to a new sterile microcentrifuge tube with 360 µL 7M ammonium acetate (NH40Ac). Tubes were inverted to mix and centrifuged at 12000 rpm x 5 min, 4 °C to separate the phases. The clear supernatant (approximately 580 µL) was transferred to a new sterile microcentrifuge tube and the lower organic phase, with the SDS forming a gel like substance, discarded. 0.54 volumes (approx. 315 µL) of isopropanol (SIGMA) was added and the tubes incubated at room temperature for 15 min. After incubation tubes were centrifuged at 12000 rpm x 5 min, 4 °C to pellet the DNA. The supernatant was discarded and the pellet washed twice with 1 mL 70% EtOH, centrifugation at 12000 rpm x 5 min, 4 °C, and the supernatant discarded. The pellet was allowed to air dry in a laminar flow hood before resuspending in 50 µL sterile ddH20. Additional purification of sediment and moonmilk DNA samples was performed using the CHROMA SPIN™ Columns DNA Purification Kit (CLONTECH Laboratories Inc.) reagents and protocol. DNA quality and quantity was analysed as described in Section 2.3.2.3. 76 Chapter 2: Materials and Methods 2.4.2 DGGE DGGE was conducted on four sediment samples and three moonmilk samples (SEl, SE2, SLl and SL2; ME2, ME3 and MXl; refer to Table 2.1) in accordance with a protocol developed by Powell et al. (2003). A standard control mix consisting of 5 ng µ1·1 each of genomic DNA extracts from four strains grown routinely in our laboratory and chosen because they denatured at a range of different denaturant concentrations was also used as a control and for comparisons between gels. The 165 rRNA gene fragment was amplified by PCR using the Advantage® 2 Polymerase Mix (CLONTECH Laboratories Inc.) reagents and protocol with Universal primers 907 forward (Santegoeds et al. 1998) and 1392 reverse (Ferris et al. 1996) with a GC clamp (Ferris et al. 1996). Reactions consisted of: 10 x Buffer 5µL 50 x dNTP Mix (10 mM each) 1 µL Primer 5' (10 pmol) 1 µL Primer 3' (10 pmol) 1 µL 50 x Advantage 2 Polymerase Mix 1 µL Template DNA" ill ddH20 to total volume 50 µL " Amount of template DNA added to PCR mix varied depending on the concentration of the DNA, however in most cases 1 µL was sufficient. 77 Chapter 2: Materials and Methods The touchdown thermal cycling parameters were: Initial denaturation step: 5 min 94 °C 1"1 3-step cycling: Denaturation: lmin 94°C Annealing: 1 min 65 °C (decreasing by 1 °C each cycle) Extension: 3 min 72 °C Number of cycles: 10 znd 3-step cycling: Denaturation: lmin 94°C Annealing: lmin 55 °C Extension: 2min 72 °C Number of cycles:. 20 Final extension: 4min 72 °C* *The final extension step is prolonged to 4 min to allow full extension of any partly amplified DNA fractions. DGGE was conducted using a D-Code Universal Mutation Detection System (Bio-Rad). Half the volume of PCR products were run on 6% (w /v) acrylamide gels with a denaturing gradient of 20-80% (where 100% dentaurant is 7 M urea and 40% formamide). Gels were run at 80 V for 16 hat 60 °C in 1 x TAE (40 mM Tris, 20 mM sodium acetate, 1 mM EDTA). Standards were run on either side of the gel and the outside lanes were not used. In order to obtain even heat distribution throughout the tank, the entire tank was placed on a magnetic stirring plate. Gels were stained in 1:1000 Sybergold (Molecular Probes) in the dark with gentle shaking for approximately 20 min. Gels were washed once with deionised H20 and destained with deionised H 20 for 20 min before viewing on a UV transilluminator (UVP Inc.). Single bands were excised from the gel using a sterile scalpel blade and resuspended in ddH20 in sterile microcentrifuge tube for 16S rRNA gene sequence analysis. Gel photos were scanned in and viewed with the UTHSCSA ImageTool program, developed at the Health Science Centre (University of Texas, San Antonio, TX, USA) and available on the internet (ftp:/ /maxrad6.uthscsa.edu). Best banding patterns were obtained by enhancing the contrast and greyscale of the images. The 16S rRNA gene fragment was amplified and purified from 78 Chapter 2: Materials and Methods eluted bands as previously described in Section 2.3.2.4 using the HotStarTaq™ PCR Master Mix Kit (QIAGEN) reagents and protocol with the exception that DGGE primers 907 (£) and 1392 (r) with a GC clamp were used, and 1 µL of the eluted DGGE band was directly added to the PCR mix. DGGE PCR products were directly sequenced as described in Section 2.3.2.4 using DGGE primer 907 (£) and subjected to phylogenetic analysis as described in Section 2.3.2.5. 2.4.3 Clone Library Analysis 2.4.3.1 165 rRNA gene PCR amplification, ligation and clone library construction. Clone libraries were generated from four sediment samples and three mo~nmilk samples (SEl, SE2, SLl and SL2; ME2, ME3 and MXl; refer to Table 2.1). The 16S rRNA gene fragment was amplified as described for DGGE analysis (Section 2.4.2) with universal primers, 519 forward and 1500 reverse (Stackebrandt et al. 1991) (Table 2.2). Reactions consisted of: 10 x Buffer 5µL 50 x dNTP Mix (10 mM each) 1 µL Primer 5' (50 pmol) 1 µL Primer 3' (50 pmol) 1 µL 50 x Advantage 2 Polymerase Mix 1 µL Template DNA" ill ddH20 to total volume 50 µL " Amount of template DNA added to PCR mix varied depending on the concentration of the DNA, however in most cases 1 µL was sufficient. Thermal cycling parameters were: Initial denaturation step: 15min 95 °C 3-step cycling: Denaturation: lmin 94°C Annealing: lmin 50 °C Extension: lmin 72 °C Number of cycles: 30 Final extension: 5min 72 °C* *The final extension step is prolonged to 5 rnin to allow full extension of any partly amplified DNA fractions. 79 Chapter 2: Materials and Methods PCR fragments were purified using the UltraClean™ PCR Clean-up DNA Purification Kit (MoBio Laboratories Inc.) and analysed for size and concentration as described in Section 2.3.2.3. 16S rRNA gene PCR frcigments were ligated using the pGEM® -T Easy Vector System I Kit (Promega) reagents and protocol. Ligation reactions were subjected to an overnight incubation at 4 °C to produce the maximum number of transformants. Transformation of ligation products was performed using the Epicurian Coli® XL2-Blue Ultracompetent Cells (Stratagene) reagents and protocol. Transformants were screened using blue-white colony colour selection. Aliquots (50 µL and 100 µL) of the transformation mixture were plated on Luria Broth agar plates containing 100 µg mL·1 ampicillin (SIGMA) (LB-Amp) and coated with 100 µL 1 0.1 M iso-propyl-beta-D-thio-galactopyranoside (120 mg mL- ) (IPTG) (SIGMA) and 20 µL 5- 1 bromo-4-chloro-3-indoyl-beta-D-thio-galactopyranoside (50 mg mL- ) (X-gal) (SIGMA) (see Appendix 1). Plates were incubated overnight for 16-20 hat 37 °C. Colonies containing recombinant plasmids with the 16S rRNA gene fragment appear white, whereas colonies containing un-recombinant colonies appear blue. Appr~ximately 150 white colonies from each library were sub-cultured to LB-Amp plates and re-incubated overnight at 37 °C. 2.4.3.2 Restriction Fragment Length Polymorphism screening and 165 rRNA gene sequencing of clones Recombinant plasmids were extracted and purified from transformed cells using the UltraClean™ Mini Plasmid Prep Kit (Mo Bio Laboratories Inc.) reagents and protocol. Plasmids were electrophoresed in a 1 % (w /v) agarose gel, 80 V x 40 min (see Section 2.3.2.2) to confirm they contained the 16S rRNA gene insert. Recombinant plasmid DNA were confirmed by correlation of their position on the gel with a plasmid known to contain the correct size insert. Plasmids containing an insert of the correct size were further screened by Restriction Fragment Length Polymorphism (RFLP) analysis. Restriction digests were performed on plasmids by separate incubation with the restriction nucleases Hinfl (New England Biolabs) and Rsal (New England Biolabs) and accompanying buffers (New England Biolabs) at 37 °C for 3-4 h. Digests were fractionated by electrophoresis on 3% (w /v) agarose gels, 100 V x 3 h, (see Section 2.3.2.2) resulting in characteristic banding patterns allowing the diversity and abundance of cloned 80 Chapter 2: Materials and Methods phylotypes to be approximated. Clones exhibiting diverse banding patterns (including 2-4 duplicate clones possessing the same RFLP pattern) were selected at random for sequencing. Clones were sequenced as described in Section 2.3.2.4 with the exception that plasmid templates were subjected to a pre-heat treatment and primers pUC/Ml3 forward and reverse were used for amplification (Promega) (see Table 2.2). Binding sites for these primers are located on the pGEM® -T Vector, positioned either side of the insert. The pre-heat treatment consisted of diluting the template with water to the appropriate concentration, heating to 96 °C for 1 min in a PTC - 200 Peltier Thermal Cycler (MJ Research), and cooling to room temperature before adding the remainder of the sequencing-reaction components. In most cases, 16S rRNA gene clones were entirely sequenced with the sequences spanning nucleotide positions 519 - 1540 (E. coli equivalent). 2.4.4 Phylogenetic and biodiversity analysis Phylogenetic analysis was conducted as described in Section 2.3.2.4 with the exception that the Ribosomal Database Project II (RDP) CHIMERA-CHECK program (http:/ /rdp.cme msu edu/; Maidak et al. 2001) was used to detect PCR-amplified hybrid sequences. In addition, potential chimeras were determined from inconsistencies in branching order. Chimerical clones detected were not included in subsequent phylogenetic or biodiversity ' analyses. For calculation of diversity indices, the libraries were normalised to 50 clones using the rarefaction method (Simberloff, 1972) by utilising the program RAREFACT.FOR written by C. J. Krebs (University of British Columbia) and which is available through the internet (http://www2.biology.ualberta.ca/jbrzusto/rarefact.php). 81 Chapter 2: Materials and Methods Estimates of Diversity (H) were determined using the Shannon-Weaver (or Shannon- Weiner) Index (Krebs, 1989). H' is given by the formula: k H' = n log n - L N log N i=l n where k is the total number of unique phylotypes, n is the total number of clones and N is the number of observations of each phylotype (i). Measures of dominance concentration were determined using the Simpson Index (SI) (Krebs, 1989). SI' is given by the formula: k SI'= L Ni ( Ni - 1 ) i = 1 n(n-1) Equitability indices (JJ were based on Shannon-Weaver index data. J' is given by the formula: ]'= H' Hmax Where H max is equal to log k. Biodiversity coverage (C) (Mullins et al. 1995) was derived by the formula: C=l-l!!J N Where ni is the number of phylotypes containing only one clone, and N is the total number of clones. Pairwise comparisons of clone libraries were carried out using the Similarity Coefficient (S) (Odum, 1971). Sis derived from the formula: S=2C A+B Where A and B are the number of phylotypes in libraries A and B respectively, and C is the number of shared phylotypes. 82 Chapter 3: Results and Discussion Chapter 3: Results and Discussion 3.1 Microscopy and Mineralogy Putative moonmilk samples were collected from an extensive speleothemic deposit in the dark zone of Exit Cave (MXl) and white mat-like material on the ceiling rock of Entrance Cave within the twilight zone (ME2). During the course of this study large moonmilk-like deposits were found beneath sediment in Entrance Cave (MEI, ME3) and analysed for comparison. ESEM with X-Ray Microanalysis was employed to investigate the microbe-mineral interface of moonmilk samples. The samples collected from the ceiling of Entrance Cave (ME2) exhibited distinct, isolated areas of thin white material on the muddy rock surface (Figure 3.2; A). X-Ray microanalysis of this material (Figure 3.1; A, B) revealed high levels of silicon and aluminium suggesting a day-type mud and high levels of carbon and oxygen suggesting areas of organic material. Figure 3.2 (B) illustrates that the isolated areas of white material on the mud surface from ME2 contained a crystalline character associated with biological growth of hyphal material. In the dark zone of Lechuguilla Cave CaC03-mineralised organic filaments have been reported (Cunningham et al. 1995). High magnification of the mat demonstrated the presence of hyphae forming microorganisms with segmented hyphae of width 0.5-1 µm, consistent in size and morphology with filamentous actinomycetes. Non-biological (crystalline) structures were evident both beneath the mat of hyphal growth and also encrusting individual hyphae. Putative cells and an organic matrix can be frequently seen in moonmilk samples with SEM or in thin sections, but not in all cases (Northup et al. 2000). Biological material or cells were not evident in ESEM analysis of moonmilk samples ME3 or MXl, though CYBR staining confirmed the presence of DNA in the samples (data not shown). 83 Chapter 3: Results and Discussion Si 0 0 a Figure 3.1: X-Ray microanalysis spectra of sample ME2 from the ceiling rock in the twilight zone of Entrance Cave. (A) Spectra of mud containing high levels of silicon, oxygen and aluminium consistent with a clay-type mud. (B) Spectra of mat sample ME2, illustrating the presence of organic material, indicated by high levels of carbon and oxygen. For the purpose of distinguishing mondmilch from other carbonate speleothems, Fischer (1988) defined true calcite moonmilk as a calcite microcrystalline or needle-crystalline speleothem with a minimum calcite content of 90 % weight. ESEM of samples MXl and the crystalline areas of ME2 (Figure 3.3) shows the needle-fibre crystalline characteristics of the calcite (confirmed by X-Ray microanalysis, data not shown). XRD studies revealed that the mineralogical composition of moonmilk samples from both Entrance Cave and Exit Cave were almost identical (Table 3.1). Moonmilk samples consisted predominantly (85-100%) of calcite (Ca03), with trace amounts of quartz, mica (clay, most likely illite) and hydrated iron oxide, goethite [oc-FeO(OH)]. Table 3.1: X-Ray Diffraction analysis of moonmilk samples from Entrance Cave, ME2 and ME3, and Exit Cave, MXl. Approximate mineralogy recorded as % weight. Sample Calcite Quartz Mica* Goethite ME2 85 3 10 2 ME3 100 MXl 100 •Probably illite. Note: Peak overlap may interfere with identifications and quantifications. Minerals present in trace amounts may not be detected. 84 Chapter 3: Results and Discussion Figure 3.2: Photographs and ESEM pictures of cave sample ME2 showing biological hyphal material and calcite encrusted hyphae. (A) White mat with reflective droplets on ceiling of Entrance Cave (ME2). B-F: ESEM images of sample ME2. (B) Mat of microbial growth on the ceiling. (Q Oumps of hyphae encrusted with calcite and uncalcified hyphae on the surrounding mud. ESEM images of calcite encrusted microbial filaments at high magnification. (D) Detailed view illustrating different degrees of encrustation exhibited by hyphae. (E) Detailed view of calcite encrusted hyphae. (F) Segmented hyphae, width approx. 0.5-1 µrn. 85 Chapter 3: Results and Discussion Figure 3.3: ESEM images of moonmilk samples illustrating microcrystalline, needle-fibre form of CaC03 crystals (confirmed by X-Ray microanalysis, data not shown). (A) Sample ME2 from Entrance Cave. (B) Sample MXl from Exit Cave. XRD and ESEM results indicate that samples MEI, 3 and MXl are true calcite moonrnilk (98-100% CaC03). Sample ME2 had a slightly lower calcite composition (85%). The thin, mat-like nature of this sample from the ceiling of Entrance Cave made it difficult to collect samples from just the white material and inevitably some of the clay layer (2-3mm thick) on the ceiling was collected too, perhaps accounting for the higher clay content (10 %) of this sample 3.2 Method Development for Calcite Moonmilk Samples It has previously been suggested that DNA extraction from environmental samples containing high levels of CaC03 is problematic (Guthrie et al. 2000; Northup, pers. comm. 2001). Initial clone analysis of samples ME2, ME3 and MXl, that have high calcite content (85-100%) as demonstrated by XRD analysis, (Section 3.1) resulted in a single phylotype most closely related to y-Proteobacteria, Pseudomonas fluorescens. Isolations also proved to be problematic initially producing almost pure cultures of Bosea thiooxidans. Though these organisms were dominant components of the calcite-based microbial communities (Table 3.2), ESEM results depicting hyphal organisms indicated that these results were not necessarily representative of the true diversity. DNA extraction methods and cultivation procedures rely on the bacterial cells being readily released from their environmental matrix. Current DNA extraction protocols for 86 Chapter 3: Results and Discussion molecular analyses are poorly adapted for lithic or encrusted microbial communities due mostly to the hard, usually cemented nature of the mineral matrix (Wade & Garcia-Pichel, 2003). Guthrie et al. (2000) suggested that as DNA was released from coral matrices it was adsorbed by the calcite minerals resulting in very low quantities of DNA being recovered. A significant portion of this study was directed at method development to enhance DNA extraction and cultivation procedures for calcite cave samples. A comparison of three DNA extraction protocols was undertaken: a modified protocol from Purdy et al. (1996) utilised for cave sediments in this study, the protocol from Guthrie et al. (2000) which was successful for coral samples, and a modified protocol from Miller et al. (1999), the Phosphate, SDS, Chloroform-Bead Beater method (PSC-B) which was successful with pure opal-A silica sinter samples (pers. comm. Dr. Susan Turner, University of Auckland, 2003). DGGE analysis of PCR amplified 165 rRNA gene from DNA product of the three extraction protocols was used to determine which method was most appropriate. PCR product resulting from the modified PSC-B DNA extraction displayed the highest degree of diversity in the banding pattern for all samples (Figure 3.4). Thus this protocol was utilised for further clone library analysis. 35% 65% ME3 ME2 ME3 ME2 Figure 3.4: 165 rRNA gene DGGE community fingerprint of Entrance Cave moonmilk samples, ME2 and ME3. (A) DNA extraction using PSC-B method. (B) DNA extraction using Guthrie et al. (2000) coral method. Illustrates the greater diversity of banding patterns for DNA extracted using PSC-B method. 87 Chapter 3: Results and Discussion Microbes were isolated from moonmilk using a modified version of an isolation procedure developed by Olivier Braissant (pers. comm. Universite de Neuchatel, Germany, 2002). Calcite samples were subjected to one of five different treatments to dissolve the carbonate and free bacterial cells for cultivation: 1) 5% acetic acid (CH3COOH) in 0.01 M MgS04.7H20 2) 1% acetic acid in O.OlM MgS04.7Hz0 3) 1 mM Ethylenediaminetetraacetic Acid (EDTA) 4) 0.1 mM EDTA 5) ddH20 (control) The 1% acetic acid and lmM EDTA treatments produced the greatest number of different colony morphology types on primary isolation plates (data not shown). The 0.1 mM EDTA and ddH20 treatments resulted in far fewer colonies and only a limited number of colony morphologies on isolation plates, indicating that these treatments did not sufficiently separate the cells from the calcite matrix. The 5% acetic acid treatment produced the least number of colonies on primary plates possibly due to the acid being bacteriocidal at this concentration. It is recognised that the application of EDTA and acetic acid solutio.ns may have introduced unknown degrees of bias to the resulting isolations. However, as it was necessary to dissolve the carbonate to obtain greater diversity in isolations, this bias was unavoidable. 88 Chapter 3: Results and Discussion 3.3 Phylogenetic Diversity Overview 165 rRNA gene clone libraries were constructed from D~\JA extracted from four sediment samples (SEl, SE2, SLl and SL2) and three moonmilk samples (ME2, ME3 and MXl). Libraries were constructed with universal primers. Approximately 100-120 clones per library were screened by analysis of RFLP patterns and selected representatives of novel RFLP patterns were sequenced. Sequences greater than 500 base pairs (bp) were included in phylogenetic analysis. Groups of two or more highly related sequences (~ 98% sequence identity) were considered to belong to the same sequence type designated a phylotype. From a total of 488 nonchimeric clones analysed from seven libraries, 148 phylotypes were defined affiliated with the domain Bacteria. A total of 43 phylotypes were found in two or more libraries. Table 3.2 provides a summary of the representative sequences and their phylogenetic affiliations. The majority of clones fell into three major phylogenetic groups: the Proteobacteria (dominating all samples), the high G+C Gram-positive Actinobacteria, and the Cytophaga-Flavobacterium Bacteroides (CFB) group. DGGE and subsequent 165 rRNA gene sequencing of bands was used to analyse moonmilk samples for comparison to clone library results. DGGE was also applied to sediment samples however the greater species diversity from sediments made the accurate defining of individual bands for sequencing difficult, a common result for sediment samples. Common banding patterns between samples indicate common community representatives. A total of six major bands present in moonmilk samples were sequenced and phylogenetically aligned with the a-Proteobacteria, Actinobacteria and CFBs. Cultures were isolated from four sediment and three moonmilk samples and from swabs of speleothems in Entrance and Loons Caves to investigate culturable diversity (see Table 2.1 for sample locations). Sediment sites were chosen away from main pathways in the dark zone of the caves and covering a range of sediment types from two caves of different character: Entrance Cave (SEl - dry sediment, SE2 - saturated sediment) and Loons Cave (SLl - dry sediment, SL2 - saturated sediment). Moonmilk samples were chosen to include two cave types (Entrance and Exit) and cover a range of forms, speleothemic (MXl), mat-like (ME2) an~ floor 89 Chapter 3: Results and Discussion deposit (ME3). Selective procedures and media favouring actinomycete growth were applied to sediment and speleothem samples whereas non-selective procedures and media were used for moonmilk samples. Gross morphology was used to discard duplicate cultures and isolates displaying novel morphology were identified using 165 rRNA gene sequencing and phylogenetic analysis. Groups of two or more highly related sequences (:::: 97.5% identical) were considered to belong to the same species in accordance with the definition of a bacterial species (Goebel & Stackebrandt, 1994; Vandamme et al. 1996). A total of 302 isolates belonging to 39 genera were sequenced, mostly belonging to the order Actinomycetales. Table 3.3 summarises the phylogenetic affiliations of representative isolates. The majority of actinomycete isolates from all samples belonged to the Streptomycineae, Pseudonocardineae, Corynebacterineae and Micrococcineae. Isolates from moonmilk samples belonged to the Actinomycetales, Firmicutes, Proteobacteria and CFB groups. 90 Cha2ter 3: Results and Discussion Table 3.2: Summary of Phylotype* Abundance and Phylogenetic Affiliations from Cave Microhabitats PHYLOTYPEA NEAREST TAXON (% IDENTITY)8 ABUNDANCE IN MICROHABITATc SEl SE2 SLl SL2 ME2 ME3 MXl D BACTERIA a-Proteobacteria Caulobacterales Caulobacteraceae ME30021 Nztrobacteria hamadamenszs AY569007 (93.9%) 1 MON0045 Brevundzmonas alba AJ227785 (94.6%) 1 1 CAVOOOl Brevundzmonas alba AJ227785 (98.2%) 7 1 2 DMONl Brevundzmonas alba AJ227785 (98.2%) -./ -./ -./ Rhizobiales Beijerinckiaceae MX10051 Methylocella palustrzs Y17144 (89.1%) 4 Bradyrhizobiaceae ME20020 Bradyrhzzobzum japomcum AF363150 (98.2%) 3 CAV0002 Bosea thiooxzdans X81044 (99.8%) 2 4 14 1 DMON2 Bosea thzooxzdans X81044 (99.8%) -./ -./ MX10048 Bosea thzooxzdans X81044 (90%) 1 5120043 Afipm masszlzenszs AY029562 (95.1 %) 2 MX10021 Afipm genosp 9 U87780 (99.2%) 1 CAV0008 Rhodopseudomonas palustrzs D12700 (93.7%) 2 2 1 Brucellaceae 5120011 Ochrobactrum anthropz U70978 (94.2%) 1 Hyphomicrobiaceae ME20041 Hyphomzcrobzum sulfomvorans AF235089 (93.8%) 1 5ED0019 Hyphomzcrobium vulgare X53182 (91.9%) 1 1 1 5110054 Devosza rzboflavma AY512822 (99.6%) 1 2 Methylobacteriaceae 5E10044 Methylobacterzum extorquens 120847 (91.1 % ) 1 Phyllobactenaceae 5E20001 Phyllobacterium myrsznacearum AJ011330 (99.2%) 2 1 1 ME20015 Ammobacter mzgataenszs AJ011761 (96.1 %) 1 Rhizobiaceae MX10017 Rhizobium gzardmn U86344 (99.1 %) 1 Rhodobacterales Rhodobacteriaceae 5120056 Rhodobacter azotoformans D70846 (97%) 1 MX10016 Rhodobacter sphaeroides D16424 (98.4%) 1 5E10043 Amarzcoccus macauenszs U88042 (85.7%) 1 5PE008 Paracoccus solventzvorans AY014175 (??%) Sphingomonadales 5E10056 Sphingomonas aerolata AJ429240 (97.5%) 1 MON0003 Sphmgomonas phyllosphaerae AY453855 (97.1 %) 1 1 CAV0009 Sphingopyxzs alaskensisAF378795 (94.2%) 1 2 2 5 1 DMON3 Sphzngopyxzs alaskenszsAF378795 (93%) -./ -./ f3-Proteobacteria Burkholderiales Acaligenaceae 5120039 Derxza gummosa (91.6%) 1 3 5E20024 Bordetella pertussis AF366576 (91.4%) 1 Burkholderiaceae 5110008 Burkholderia sordidicola AF512827 (92.9%) 4 5110014 Limnobacter thiooxidans AJ289885 (89.2%) 1 2 CAV0003 Pandorea apzsta AF139172 (93.1 %) 2 1 1 Commamonadaceae CAV0004 Hydrogenophaga defluvzi AJ585993 (94.3%) 1 2 1 5120003 Hydrogenophaga palleromz AF019073 (98.7%) 1 MX10008 Delftia tsuruhatenszs A Y302438 (97.3%) 1 MONOOlO Polaromonas vacuolata U14585 (95 7%) 1 3 5110033 Varzovorax paradoxus AJ420329 (99.3%) 1 5120010 Aczdovorax valerzanellae AJ431731 (96.1 %) 1 5E20028 Ottowia thzooxydans AJ537466 (92.4%) 1 Oxalobacteraceae CAV0005 Janthmobacter agarzczdamnosum Y08845 (98.3%) 2 2 4 3 MON0015 Masszlza timonae U54470 (97.5%) 5 4 CAV0006 Duganella vzolaceusniger AY376163 (97%) 1 5 5 ME30010 Oxalobacter formzgenes U49758 (96 3%) 1 1 CAV0021 Herbaspirzllum f!:zsmgense AJ238358 (??) 2 3 1 Continued on next page 91 Cha12ter 3: Results and Discussion PHYLOTYPEA NEARESTTAXON (% IDENTITY)8 ABUNDANCE IN MICROHABITATc SEl SE2 SLl SL2 ME2 ME3 MXl D Hydrogenophilales Hydrogenophilaceae 5110010 Thzobaczllus denitrificans AJ243144 (94.5%) 2 Methylophilales Methylophilaceae SL00008 Methylophilus leismgerz AF250333 (97.8%) 2 5 SE20011 Methylophilus freyburgenszs AJ517772 (93.3%) 8 SL00038 Methylovorus mays AY486132 (94.3%) 3 8 Nitrosomonadales Nitrosomonadaceae SL20020 Nitrosospira brzensis AY123800 (90.2%) 4 Unclassified SED0039 Thzobacter subterraneus AB180657 (89%) 1 1 &-Proteabacteria Desulfuromonadales Desulfuromonadaceae MON0018 Desulfuromonas thiophzla Y11560 (90%) 1 1 1 Geobacteraceae SE10098 Geobacter pelophzlus U96918 (91 % ) 1 Desulfoarculales Desulfoarculaceae SL0043 Nztrospma gracilis L35504 (92%) 2 2 1 y-Proteobacteria Acidithiobacillales Acidothiobacillaceae SE10004 Aczdothiobacillus ferroxzdans AJ457808 (98%) 2 Alteromonadales Alteromonadaceae SED0012 Marmo bacterium georgzense AB021408 (99%) 1 1 Chromatiales Chromatiaceae SED0017 Nztrosococcus oceanz AF363287 (91 % ) 3 1 SL10022 Nztrosococcus oceani AF363287 (90%) 1 SEDOOlO Thzocapsa roseoperscma Y12303 (93%) 3 1 SE10089 Thzobaczllus prosperus AY034139 (94%) 1 Ectothiorhodospiraceae SE10058 Thioalkalivibrio thzocyanodenztrzficans AY360060 6 (92%) Enterobacterales SED0008 Photorhabdus luminescens D78005 (95%) 9 9 2 Legionellales SE10003 Legzonella londmzenszs Z49728 (94%) 1 Methylococcales SE10021 Methylococcus capsulatus X72770 (90%) 1 ME30011 Methylococcus capsulatus X72770 (91 %) 1 Pseudomonadales CAVOOll Pseudomonas fluorescens AF094729 (98%) 1 3 2 4 3 SE20012 Pseudomonas putida AF094743 (98%) 2 SE20021 Pseudomonas angu1!11sept1ca X99540 (98%) 1 MX10050 Uncultured bacterium clone Cll-Kll AJ421116 1 (95%) Moraxellaceae ME30060 Acinetobacter 7ohnsoni1 Z93440 (94%) 2 Thwtrichales Thiotrichaceae SE20006 Achromabum oxahferum L48227 (93%) 1 Xanthomonadales SE10045 Lysobacter gummosus AB161361 (97%) 2 SE10044 Lutezmonas mephitzs AJ012228 (97%) 1 SL10051 Frauterza aurantza AJ010481 (95%) 1 SED0009 Hydrogenocarbophaga effusa AY363244 (93%) 1 2 1 CAV0030 Pseudoxanthomonas mexzcana AF273082 (96%) 1 1 1 Actinobacteria Actinobacterideae Actinomycetales Corynebacterineae ME20019 Nocardza carnea X80607 (99%) 3 2 2 ME20104 Nocardza corynebacterozdes X80615 (94%) 2 Micrococcineae MEX005 Arthrobacter chlorophenolzcus AF102267 (96%) DMON4 Arthrobacter chlorophenolzcus AF102267 (96%) -./ -./ -./ CAV0027 Arthrobacter pascens X80740 (99%) 1 2 2 2 CAV0046 Arthrobacter ox't.dans X83408 (99%) 1 2 Conbnued on next page. 92 Cha£ter 3: Results and Discussion PHYLOTYPEA NEAREST TAXON (% IDENTITY)8 ABUNDANCE IN MICROHABITATc SEl SE2 SLl SL2 ME2 ME3 MXl D SL20016 Arthrobacter psychrolactzcus AF134183 (98%) 1 MON021 Knoellza subterranea AJ294413 (99%) 3 1 1 2 Pseudonocardineae ME20021 Pseudonocardza asaccharolytzca Y08536 (95%) 3 SL10013 Actznobispora alamniphila AF325726 (96%) 1 ME20012 Amycolatopszs fastzdiosa AJ400710 (96%) 1 ME20103 Amycolatopszs sulphurea AJ293756 (96.5%) 2 ME20081 Saccharothrix coeruleofusca AF114805 (95%) 1 CAVOOlO Saccharothrix texasenszs AF350247 (97%) 2 1 1 4 MON0007 Saccharothrix cryophilzs AF114806 (95%) 4 2 3 DMON5 Saccharothrix cryophilis AF114806 (95%) -.J -.J -.J MON0018 Lentzea albidocapillata X84321 (96%) 1 SE10086 Lechevalierz aerocolonzgenes AY196703 (88%) 1 SL20046 Kzbdelosporangium phillipznense AJ512464 (95%) 1 Propionibacterineae CAV0023 Propionzbacterium acnes AB042288 (98%) 1 1 SED0051 Nocardioides fulvus AF005016 (94%) 1 2 MX10002 Nocardioides sp. LMG20237 AJ316318 (92%) 1 MX10032 Pzmelobacter simplex 278212 (98%) 1 Micromonosporineae SL10009 Micromonospora echznoaurantzaca X92618 (98%) 1 ME20061 Actznoplanes cyaneus AB036997 (95%) 1 MX10039 Virgosporangzum ochraceum AB006167 (91 % ) 2 Frankineae SE0098 Frankza sp. 2 2 SE10039 Blastococcus saxobsuiens AJ316570 (90%) 1 Streptomycineae SL10019 Streptomyces caviscabies AF112160 (99%) 2 1 1 ME20022 Streptomyces subrutilis X80825 (97%) 1 2 ME30039 Streptomyces sangl1er1 AY094364 (98%) 1 ME20033 Streptomyces vwlaceoruber AF503492 (98%) 1 SE00050 Streptomyces yunnanenszs AF346818 (91 %) 1 1 CAV0015 Streptomyces macrosporus 268099 (90%) 1 2 ME20041 Streptomyces rutgersenszs 276688 (99%) 1 SE10028 Streptomyces galzlaeus AB045878 (98%) 1 SL10055 Kitasatospora medwcidzca U93324 (97%) 1 Rubrobacterideae ME30059 Thermoleophilum minutum AJ458464 (89%) 1 ME30009 Thermoleophzlum album AJ458463 (93%) 1 Sphaerobacterideae SE10001 Sphaerobacter thermophilus AJ420142 (90%) 1 Unclassified Actinobacteria SE10060 Cand1datus Mzcrothrzx parvzcella X89774 (91 %) 2 1 Firmicutes SL10009 Ruminococcus flavefaczens X85097 (91 %) 2 MX10063 Bacillus subtilus AB042061 (99%) 1 1 ME20098 Sporosarczna ureae AF202057 (98%) 2 Cytophaga-Flavobacteria-Bacteroides Bacteroidetes Flavobacteriales Flavobacteriacea MX10045 Cryomorpha ignava AF170738 (92%) 1 SL10003 Flavobacterza ferrugzneum M62798 (96%) 1 SL10020 Flavobacterium columnare M58781 (93.3%) 1 CAV0015 Flavobacterza lzmicola AB075230 (98%) 1 2 6 8 ME30007 Flavobacterza lzmzcola AB075230 (93%) 2 CAV0018 Flavobacterza leeana AB180738 (98%) 2 3 1 1 10 DMON6 Flavobactena leeana AB180738 (98%) -.J -.J CAV0030 Antarctic bacterium R-7933 AJ440987 (97.1 %) 1 1 Sphingobacteriales Sphingobacteriaceae MON0015 Pedobacter cryconztzs AJ438170 (97%) 2 1 ME30041 Sphzngobacterzum faeczum AJ438176 (93.4%) 3 Bacteroidales Continued on next page. 93 Cha12ter 3: Results and Discussion PHYLOTYPEA NEARESTTAXON (% IDENTITY)8 ABUNDANCE IN MICROHABITATc SEl SE2 SLl SL2 ME2 ME3 MXl D SL0019 Flexibacter tructuosus M5S7S9 (92%) 1 1 SL10002 Uncultured bacterium clone C44K17 AJ297617 1 (92.9%) CAV0026 Bacteroidetes bacterium Mo-0.2plat-K3 AJ622SSS 1 1 1 (90.9%) Acidobacteria ME20061 Uncultured bacterium DADOS Y12597 (97%) 1 MON0045 Uncultured bacterium DADOS Y12597 (94%) 2 2 ME20013 Uncultured bacterium DADOS Y12597 (90%) 2 ME20020 Bactenum Ellin6075 AY234727 (94%) 1 ME20050 Bacterium Ellm6075 A Y234727 (91 %) 1 SL20005 Bacterium Ellin6071 AY234723 (95%) 1 SL10020 Bactenum Ellin52S9 AY234640 (S9%) 1 Planctomycetales SE10039 Planctomyces braszlzenszs AJ231190 (90%) 5 CAV0062 Planctomyces marzs AJ231184 (90.4%) 4 2 1 1 SED0061 Pzrellula staleyz AJ2311S3 (96%) 2 1 2 2 SE0051 Pzrellula sp. XS1947 (SS S%) 3 1 SED0047 Planctomycete str.292 AJ2311S2 (S7.2%) 2 1 1 SL10061 BacteriumDR2A-7G19 AB127S5S (91.2%) 1 ME30013 Gemmata-like str. C1uq14 AF239693 (Sl.9%) 2 Chloroflexi (green nonsulfur) ME20011 Caldilznea aerophzla AB067647(S6.4%) 2 SE0037 Caldilznea aerophzla AB067647 (90%) 1 1 MX10044 Dehalococcoides ethenogenes AF00492S (95.6%) 1 MX10041 Anaerolznea thermophzla AB046413 (91.9%) 1 ME30006 Urudentified bacterium strain BD3-16 AB015556 1 (S6.9%) Verrucomicrobia SE10094 Uncultured verrucomicrob1um DEVOlO 2 AJ401127 (92%); Verrucomzcrobza spinosum X90515 (S6.5%) SE10006 Opitutus sp VeSm13 X99392 (91.S%) 1 OP10 SL20004 Uncultured bactenum SJA-176 AJ009504 (S6%) 1 SL20017 Uncultured bacterium GC55 AJ27104S (90.2%) 1 Gemrnatimonadetes SL20096 Gemmatzmonas aurantiaca AB072735 (S7 6%) 3 SL20036 Bactenum Ellm 5301 AY234652 (S7.S%) 2 ARCHAEA Crenarchaeota SL20017 Uncultured archaeon WSB-11 AB055993 (91.S%) 1 Desulf!!:.rococcus amy_loly_tzcus AF250331 (75%) Total:# phylotypes 40 34 39 39 31 29 40 (#clones) (72) (60) (68) (68) (71) (61) (75) *Phylotypes represented m sed!IIlent and moommlk samples (CAV) Phylotypes represented in sediments of Entrance and Loons Caves (SED). Phylotypes represented m more than one moonmilk sample (MON) DGGE bands from moonmilk (DMON); presence(.../), absence(-). A A umque sequence or group of highly related sequences (> 98% identical) cous1dered to belong to the same sequence type. 8 Inferred from drrect sequence comparison to representative sequences on GENBANK. Access10n numbers given c No of clones m phylotype represented m each nucrohabitat studied based on drrect sequence comparisons or inferred from RFLP patterns 0 Microhabitats represented by samples. SE! (dry sediment, Entrance Cave), SE2 (wet sediment, Entrance Cave), SL! (dry sediment, Loons Cave), SL2 (wet sediment, Loons Cave), ME2 (calcite mat, Entrance Cave), ME3 (moonnulk, Entrance Cave), and MXl (moonmlik, Exit Cave). 94 Chapter 3: Results and Discussion Proteobacteria The Proteobacteria were the most commonly sampled group (35.2-76.5% of clones) present within the cave samples. Representatives of the alpha (a), beta(~), gamma (y) and delta (8) subclasses were detected in varying proportions in the clone libraries. No epsilon (c) Proteobacteria clones were detected in this study. a-Proteobacteria A total of 81 clones representing 24 phylotypes were affiliated with the a-Proteobacteria and representatives were detected in all libraries (Table 3.2). Three DGGE bands (DMONl, 2 and 3) affiliated with the a-Proteobacteria were present in all 3 moonmilk samples. Isolates from sediment, speleothems and moonmilk were also affiliated with the a-Proteobacteria. Figure 3.5 displays an evolutionary distance dendrogram of representatives of the a subclass and associated cave clones, DGGE bands and isolates. The most pronounced clade was the Rhizobiales consisting of 15 phylotypes from all samples affiliated with Beijerinckiaceae, Bradyrhizobiaceae, Brucellaceae, Hyphomicrobiaceae, Methylobacteriaceae, Phyllobacteriaceae and the Rhizobiaceae. The most dominant phylotype present in high numbers in both Loons sediments and all moonmilk samples (CAV0002) was most closely related to Bosea thiooxidans (99.8% sequence similarity), a thiosulfate oxidiser (Das et al. 1996). The isolation of a strain of Bosea thiooxidans and the presence of 14 clones of this phylotype in the Entrance mat material indicates that this is a major component (19.71 %) of the total microbial community. The Bosea thiooxidans phylotype was also detected in all moonmilk samples by DGGE analysis (band DMONl). A number of clones were affiliated with methylotrophic taxa (phylotypes MX10051, ME20041, SED0019, SE10044) including representatives of the genera Methylobacterium, Methylocella, and Hyphomicrobium. Phylotypes ME20041 and SED0019 formed a deep lineage within the Hyphomicrobiaceae. A novel pink pigmented Methylobacterium sp. was isolated from moonmilk and phylotypes branching with genera Methylobacterium and Methylocella were detected in Entrance sediment and moonmilk from Exit. Phylotype MX10051, consisting of four clones, formed a deep branching lineage 95 Chapter 3: Results and Discussion within the Beijerinckiaceae affiliated loosely with Methylocella paulstris (89.1 % sequence similarity). M. palustris is a methanotrophic acidophile isolated from peat wetlands (Dedysh et al. 2003). Other members of the Bezjerinckiaceae are free-living aerobic nitrogen-fixing bacteria (eg. Beijerinckia) which grow well in acidic soils. Sediment phylotypes were also affiliated with nitrogen-fixing bacteria including those usually associated with plant nodules (eg. Rhizobium, Bradyrhizobium) (Young & Haukka, 1996). The second clade of interest is the Caulobacterales. Phylotype SL20021 was affiliated with Nitrobacter sp., a facultative nitrifying chemolithotroph (Zare et al. 2003; published in database only), detected in saturated sediment from Loons but not detected in dry sediment from Loons or Entrance samples. Phylotypes affiliated with Brevundimonas sp. were detected in all moonmilk samples. MON0045 was most closely related to Brevundimonas alba (98.2%), a prosthecate oligotroph (Abraham et al. 1999), and present in particularly high numbers in sample ME2 (-10% of total community). Prosthecae are narrow extensions of the bacterial cell wall containing cytoplasm and it has been proposed that these structures confer a variety of benefits to aerobic heterotrophic bacteria including mechanisms for attachment to solid substrates and enhanced respiration and nutrient uptake (Hedlund et al. 1996). Brevundimonas alba was also present in the DGGE analysis (band DMON2) and isolated from all moonmilk samples, reinforcing its ubiquity in moonmilk. Members of the Sphingomonadales were detected in sediments and moonmilk samples. Particularly, phylotype CAV0009 most closely related to Sphingopyxis alaskensis (94.2%) was detected in all samples except for SLl and was detected in DGGE analysis (DMON3). Putatively novel members of the genus Sphingomonas and Sphingopyxis were also isolated from sediments (SEEOOS) and moonmilk (MAE322). Members of the Sphingomonadales are oligotrophic and found in nutrient limited subsurface environments where they metabolise a large number of aromatic compounds (Fredrickson et al. 1995 Balkwill et al. 1997; Barton et al. 2004). Such metabolic diversity has led to the identification of members of this genus in numerous starved environments including distilled waters and oligotrophic marine ecosystems (Balkwill et al. 96 Chapter 3: Results and Discussion 1997). A novel Porphyrobacter sp. was isolated from moonmilk (MEE338). Members of the Porphyrobacter are aerobic and photosynthetic bacteria. Three phylotypes and one isolate clustered within the Rhodobacterales lineage. Two phylotypes from moonmilk (MX10016) and Loons sediment (SL20056) were affiliated with phototrophic Rhodobacter sp. A third phylotype SE10043 from Entrance sediment was loosely affiliated (85.7% sequence similarity) with members of the genera Amaricoccus, isolated from activated sludge. A novel methylotroph from the Rhodobacterales lineage, Paracoccus sp., was isolated from a speleothem in Entrance Cave. Paracoccus sp. can utilise methylamine and methyl formamide (Urakami et al. 1990). 97 Chapter 3: Results and Discussion .------My.wcoccusjulvus A1233917 L AF3'l20'JI --c======ComaTTWnasEscherCf:h"Wc~f.JMl/~uni lts/osleroni Ml 1224 ..------Riclieltsia pr Rltodoba.cterales 0.1 Figure 3.5: Phylogenetic dendrogram illustrating the evolutionary relationship between cave taxa and members of the a Proteobacteria. The dendrogram was constructed from an alignment of 1000 nucleotide pa;itions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Tltem1oprotei1s te11ax was used as the outgroup species. The scale bar indicates 10% sequence divergence. Colour Code: Black = Clone sequences, Blue = DGGE sequences, Brown = Isolate sequences. 98 Chapter 3: Results and Discussion ~ Proteobacteria Clones affiliated with the ~-Proteobacteria were the most abundant group detected in this study (102 sequences) and were distributed fairly evenly between sample sites SE2, SLl, SL2, ME3 and MXl contributing approximately 25-34% to the total diversity sampled (Table 3.2). In comparison however, no ~-Proteobacteria were detected from sites SEl or ME2. Phylotypes affiliated with the ~-Proteobacteria are depicted in Figure 3.6, clustering with known chemolithotrophs, particularly hydrogen utilising bacteria, thiosulfate oxidisers, and nitrogen-fixing bacteria. Most phylotypes clustered within the Order Burkholderiales. Several sequences obtained from both sediment and moonrnilk were closely related (94-99.3% sequence similarity) to members of the Commamonadaceae, particularly the Acidovorax group, including the genera Acidovorax, Variovorax, Polaromonas, and Hydrogenophaga. DGGE analysis also detected a member of the Hydrogenophaga in ME3 and MXl (DMON4). A novel Acaligenes sp. (MEE109) was isolated from moonmilk. Members of the Commamonadaceae and Acaligenaceae are aerobic chemoorganotrophs and some strains are capable of chemolithoautotrophy utilising hydrogen as an energy source. Nitrogen-fixation has been reported for some genera, eg. Burkholderia, Derxia and Hydrogenophaga (Willems et al. 1991). Phylotypes from sediment and moonmilk were distantly related to members of thiosulfate oxidising genera Thiobacillus, Limnobacter, Ottowia and Delftia (eg. Spring et al. 2001). A number of clones from moonmilk samples were distributed within five phylotypes affiliated with the Oxalobacteraceae, showing close relationships (>96%) with the genera fanthinobacter, Massilia, Duganella, Oxalobacter and Herbaspirillum. A number of members of the Oxalobacter group are nitrogen-fixing bacteria associated with plants (Valverde et al. 2003). Members of one genus Duganella are also reported to have chitinolytic properties, most likely associated with the breakdown of organic matter. The Oxalobacteriaceae appear to be a dominant component of the true calcite moonmilk microbial communities sampled accounting for 24% and 18% of samples ME3 and MXl, respectively. Further evidence of this is the presence of DGGE band DMON6 clustering withfanthinobacter phylotypes. 99 Chapter 3: Results and Discussion Phylotypes affiliated with the Methylophilales dominated the sediment samples, particularly the saturated sediments from Entrance and Loons Cave. SE20011, most closely related to Methylophilus freyburgensis (93.3% sequence similarity) accounts for 13% of the sampled microbial community in saturated sediment from Entrance Cave. Members of the Methylophilus genus are methanol utilising. SL00038 most closely related to Methylovorus mays (94.3% sequence similarity) accounts for 18% of the observed microbial community in saturated sediment from Loons Cave. Members of the Methylovorus are aerobic obligate methylotrophs associated with plants (Doronina et al. 2000). A single phylotype (SL20020) from saturated Loons sediment grouped with the ammonia-oxidising species Nitrosospira briensis (90.2%). c5- Proteobacteria Clones affiliated with the o-Proteobacteria were detected in all samples. This phylum encompasses sulfate- and sulfide-reducers that are morphologically diverse and obligate anaerobes. Six clones were distributed among three phylotypes (Table 3.2), thus the o Proteobacteria were a minor, though ubiquitous component of the microbial communities sampled. Two types of sulfate-reducers are recognised, those species that reduce sulfate to hydrogen sulfide (H2S) (eg. Desulfovibrio, Desulfomonas, Desulfotomaculum, Desulfobulbus) and those that reduce sulfate to sulfide (eg. Desulfobacter, Desulfococcus, Desulfosarcina, Desulfonema). Two phylotypes formed separate deep branching lineages within the Desulfuromonadales (Figure 3.7). MON0018 was detected in all moonmilk samples and represents a putatively novel lineage forming a monophyletic clade with the genus Desulfuromonas (90% sequence similarity to Desulfuromonas thiophila). Members of this genus are obligate sulfate-reducers and widespread in terrestrial and aquatic environments that become anoxic as a result of microbial decomposition processes (Finster et al. 1997). Phylotype SED0098 present in sediment samples SE2, SLl and SL2 were affiliated with sulfur- and iron- reducing members of the Geobacteraceae. A third phylotype SE10043 detected in sample SEl, formed a deep branching lineage within the Desulfoarculaceae. The closest cultured relative to this clone was nitrite-oxidiser Nitrospina gracilis. 100 Chapter 3: Results and Discussion a ,.------Rickettsia prowazekii M21789 .______Campylobacter jejw1i AF372091 E y ..------Escherichia coli X80725 Nilrosospira brie11Sis AY123800 Nitrosomonadales SL20020 Meth.vlophilusfreyb11rf1.e11Sis AJ517772 Methy/ophi/11s 111ethylotrop/u1s Ll5475 Methylophi/11s /eisi11geri AF250333 Methylophilales SL0008 .----SL0038 Methvlovor11s mays AY486132 Burkholderia sordidico/a AF512827 · SL10008 Burkholderaceae .------SL10014 Der.J.ia g11111111osaAB08948l ME20024 Acali!1,e11es faecalis D88008 Acaligenaceae Acalige11es sp. 2-6 A Y296717 CAVI109 Bordetella pertussis AF366576 Achro111obacter xvlosoxida11s AF510042 D11ga11ella violace~s11iger A Y376163 CAV0006 ME30010 Oxalobacter formige11es U49758 Oxalobacteraceae Ja11thi11obacter a.~aricida1111ws11111 Y08845 DMONS CAVOOOS Oxalobacter for111i11e11es U49758 CAV0021 Herbaspirillw11 frisi11. ~e11se AJ238358 Stero/ibacteriw11 de11itrifica11s strain Chol-ls AJ306683 Co111a111011as testosteroni Ml 1224 Delftia tsur11hate11sis A Y302438 MX10008 Acidovorax valeria11e/lae AJ431731 Po/aro111011as vacuolata U14585 Glacier bacterium FJS31 AY315178 Co11u11amo11adaceae MONOOlO Hydro11e11opha .~a defl11vii AJ585993 Arsenite-oxidising bacterium AY027499 CAV0004 DMON4 Ottowia thioo.J.vdans AJ537466 SE20028 Thiobacillus de11itrifica11s AJ243144 SL10010 Hydroge11ophilales 0.1 Figure 3.6: Phylogenetic dendrogram illustrating the evolutionary relationship between cave taxa and members of the {3- Proteobacteria. The dendrogram was constructed from an alignment of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Thennoproteus te11a.x was used as the outgroup species. The scale bar indicates 10% sequence divergence. Colour Code: Black =Clone sequences, Blue = DGGE sequences, Brown = Isolate sequences. 101 Chapter 3: Results and Discussion ...------Thermoproleustena.t:r-..f35966 ...------Esc11cncl11a coll X80725 y ~------Comamo11as le.stoJ,1erom M11224 ~ a ...------Ru.kettsmprcrn-a::.eku M21789 ...------Campvlolxu:ter Jf!JU!lt AF372091 Desulfurel/a/cs '------Desulfurella aceln1oraus X72768 ...------Bdellov1bno bactenovoms M59297 Bdellowbrw11ales ..------MJ\OCOCCllSfufrus A1233917 1\fy}.OCOCCales ...------N11rospma gracrlls 1.35504 '------SL0043 ...------Desulfobacler postgaler AF418180 Umdenb.fied su]fate reducmg bactenum DSB-Dsa99-4 AJ300510 Desulfobacteralcs Desulfo11ema 11m1cola U45990 Desulfococcus mulllvorans AF418173 Desulfococws bwt1wtus i\J217'8ff7 Desulfuramonas m.J?lotuiafls l\12~ Dr.sulfuromona.s palm1talls U28172 Desulfuromonas tluoplula Y11560 Desulfaromonadales .______MON0018 Pelobacter mas11el1enszs A Y 187308 Pelobacteracrd1galhc1 s.tram MaGa12-T X77216 SE10098 Geobacter peloplnl11s U96918 Geobaclc>r h111rureduce11s AY187306 ...----- Desulfomomle uedpn :M26635 Sw10tropliobac1erv,,o/11nr X10905 Syntrophobactera/ es Dcsulfurolwbdus ammgemts X83274 01 Figure 3.7: Phylogenetic deudrogram tllustratmg the evolutionary relauonsh1p betwe.en cave ta"Xa and members of the 0-Proteobactena The dendrogram was constructed from an ahgnment of 1000 nucleotide positions Distances were calculated m DNADIST and trees \\ere inferred h} the ne1ghbour-101mng method Thermoproteus te11cu was used as the outgroup species The scale bar mdicates 10% sequence divergence r-Proteobacteria A total of 77 clones in 22 phylotypes were affiliated with the y-Proteobacteria. Figure 3.8 illustrates the phylogenetic distribution of y-phylotypes. The y-Proteobacteria dominated Entrance sediments SEl and SE2 representing 29.6% and 26.2%, respectively, of the diversity sampled and also represented a significant component of sample SLl (21.8%) (Table 3.2). Several sequences from Entrance sediment SEl clustered within the Order Chromatiales, whose members 102 Chapter 3: Results and Discussion are predominantly phototrophic and includes sulfur-, H 2S- and thiosulfate- and nitrite-oxidising autotrophic genera Nitrosococcus, Thioalkalivibrio, Thioploca, Beggiatoa. Some cultured representatives are capable of utilising atmospheric C02 as a carbon source for growth in dark conditions. SEl clones affiliated with the Chromatiales represent 19% of total diversity sampled thus inferring that these are a dominant component of the community. SE10058, consisting of six clones, was affiliated with Thioalkalivibrio thiocyanodenitrificans (92% sequence similarity) an obligate sulfur-oxidising/ nitrifying chemolithoautotroph. Two phylotypes distantly related to autotrophic denitrifyer species Nitrosococcus oceani (90-91 % sequence similarity) were detected in both Loons and Entrance sediment. Phylotype SEDOOlO, also detected in both Entrance and Loons sediment clustered with Thiocapsa roseoperscina, a thiosulfate-oxidiser. The Pseudomonads (Pseudomonadales and Xanthomonadales) are a diverse group of aerobic chemoheterotrophs that never show fermentative metabolism. Some members are chemolithotrophic using H 2 and CO as sole electron donors and some members can use nitrate as an electron donor. Within the Pseudomonadales, a number of sequences, distributed in four phylotypes, from sediments and moonmilk clustered with the genus Pseudomonas, most closely related to members of the fluorescent sub-group (P. fluorescens, P.putida, and P.aeruginosa) and a single phylotype from moonmilk clustered with Acinetobacter. Pseudomonads have simple nutritional requirements, the most striking feature being a versatile metabolic lifestyle and the ability to metabolise a range of substrates including numerous aromatic compounds as the sole carbon and energy source. Several clones were distributed amongst five phylotypes showing high sequence similarity (95-97%) with denitrifying genera of the Xanthomonadales, (Lysobacter, Luteimonas, Frauteria, Hydrogenocarboniphaga, Pseudoxanthomonas) and a novel Xanthomonas sp. was isolated from moonmilk. Xanthomonadales are also ecologically important in soil and water and are probably responsible for degradation of many soluble compounds derived from the breakdown of plant and animal materials in oxic environments (eg. Lysobacter sp. can lyse both bacteria and fungi through array of lytic enzymes). A second novel Xanthomonad was isolated from moonmilk, the closest cultured relative being Stenotrophomonas maltophilia, which is also the 103 Chapter 3: Results and Discussion closest relative of clones of novel iron-oxidising bacteria (Emerson & Moyer, 1997). Rice et al. (1995) also found that S.maltophilia studied in biofilms showed exceptionally adhesive and corrosive properties. Phylotype SED0008 from sediment samples SE2, SLl and 2, clustered with the Enteric bacteria, a homogenous, facultatively aerobic, group within y-Proteobacteria. This phylotype was numerically significant in that it contained nine clones from SE2 and SLl, and 2 clones from SL2. Phylogenetically, it was most closely related to both Photorhabdus luminescens and Escherichia coli strain 5.1. P.luminescens is a symbiotic bacteria and E.coli is able to grow on a wide variety of carbon and energy sources. Other minor components of the y-Proteobacteria clones include, a phylotype (SE20006) closely related to Achromatium oxaliferum (93%) a sulfur-oxidiser that has sulfur and calcite inclusions within the cell, detected in Entrance sediment. Phylotypes, SE10021 and ME30011, were distantly affiliated (90-91 %) with Methylococcus capsulatus, a methane dependant bacteria. SE10004 was closely related to Acidothiobacillus ferroxidans (98%) a ubiquitously distributed chemolithotroph that derives energy from reduced sulfur compounds or by oxidising ferrous iron to ferric iron (Kelly & Wood, 2000). Aferroxidans is also capable of autotrophic growth by C02 fixation. No y-Proteobacteria clones were detected in sample ME2 or in DGGE analysis. 104 Chapter 3: Results and Discussion Rickettsia prowazekii M21789 a ..------Campylobacterjejuni AF372091 e Myxococcus f11/vus AJ233917 a .------Co111amo11as testosteroni Ml 1224 y '------Dichelobacter 11odosr1s M35016 .-----SE10004 ._____ Acidithiobacillus ferrooxidalls AJ457808 AcidithiobacilJales SE1004S Lysobacter g11111111os11S AB161361 Ste11otrooho111011as 11ilritireduce11s Ste11otropho111011as maltophi/a X95923 CAVIUO Xanthomonadales Fra111eria a11ra111ia AJ010481 SLlOOSl Ni1rosococc11s halophi/11s AJ298748 Nilrosococc11s occa11i AF363287 SED0007 Chromatiales SL10022 .---- Aero111011as 1110/111scon1111 A Y 532692 .------Vibrio cltolerae X76337 .------Pasteurella 11111/tocida Escheric/1ia co/i X80725 Esc/1eric/1ia co/i str.5.2 AY319393 SED0008 Enterobacterales P/10/orhalxius /11111i11esce11s 078005 Silieella fle.rncri X96963 ...--- - Ac/1ro111ati11111 oxalifen1111 L48227 '------SE20006 Legio11e//a /011di11ie11sis Z49728 SEHl003 Le11io11el/ales Me1hvlococc11s caps11lat11s X72770 '-----L_ __Jr-- ME30011 Metftylococcales SE10021 ..---- Nitrococcus mobilis 135510 Alkalispiril/11111 mobile AF114783 SEDOOlO Thiobacil/11s prospems AY034139 Chromatiales Th ioalcalovibrio 11itra1us AF126547 Uncultured bacteriwn clone Cll-Kll Thioalkalivibrio thiocva1uxiP11i1rifica11s AY360060 Pse11do111011as f11wresce11s AF094729 SE20012 Pse11do111oll(IS p111ida AF094743 Pseudo111011adales SE20013 Pser.1do111011as a11g11i/lisep1ica X99540 Mari11obac1eri11111 georgiense AB021408 SED0012 0.1 Figure 3.8: Phylogenetic dendrogram illustrating the evolutionary relationship between cave taxa aud members of the y Proteobacteria. The dendrogram was constructed from au aligmnent of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Themwproteus te11ax was used as the outgroup species. The scale bar indicates 10% sequence divergence. Colour Code: Black = Clone sequences, Brown = Isolate sequences. 105 Chapter 3: Results and Discussion Actinobacteria The Actinobacteria were the second most commonly sampled group overall behind the 13- Proteobacteria though not always the second most abundant group in individual libraries. Unlike the 13-Proteobacteria, phylotypes affiliated with the Actinobacteria were detected in all sediment and moonmilk samples. A total of 85 clones were distributed among 37 phylotypes illustrating the broad diversity of Actinobacteria sampled in this study (Table 3.2). Particularly, the Actinobacteria were the second most abundant group in sediment sample SEl and mat sample ME2, both from Entrance Cave, composing 36.6% and 26.8%, respectively, of the total sampled clonal diversity. DGGE analysis revealed two Actinobacteria taxa in moonmilk samples, DMON6 and DMON7 (Table 3.2). Isolations from sediments, speleothems and moonmilk samples were dominated by Actinobacteria resulting in cultured representatives from 14 genera, including one putatively novel genus and five putatively novel species (Table 3.3). The Pseudonocardineae dominated the clone libraries and revealed great diversity. A total of ten phylotypes were detected (Figure 3.9) and were particularly abundant in calcite sample ME2 with 6 phylotypes consisting of 15 clones. Several sequences from sediment and moonmilk were affiliated with the genus Saccharothrix most closely related to various described species. 17% of the total diversity sampled in ME2 were affiliated with Saccharothrix species illustrating the dominance of this taxa in the calcite samples. DGGE analysis also revealed the presence of Saccharothrix sp. in calcite moonmilk samples (DMON5). Saccharothrix sp. were isolated from moonmilk and sediment, including S.albidocapillate, S.cryophilus and S.violacea. S. violacea is a chemoorganotrophic strict aerobe that was isolated from soils inside a gold mine cave in Korea (Lee et al. 2000) and has been detected in other caves (Schabereiter-Gurtner et al. 2002, 2004; Northup et al. 2003). A novel Amycolatopsis sp. was isolated from sediment from Entrance Cave. Clones and isolates affiliated with the genera Micromonospora, Couchioplanes and Actinoplanes were also present from sediments and moonmilk. Sequences clustering within the Propionibacterineae were detected in sediment and moonmilk samples (Figure 3.9). A phylotype closely related to Propionibacterium acnes (98%), a common human skin commensal, is probably a contaminant. Clones related to Nocardioides fulvus (94% sequence similarity) and Pimelobacter 106 Chapter 3: Results and Discussion simplex (98%) were detected in sediment and calcite samples. Members of the Nocardioides are oligotrophic and able to support growth on a wide variety of substrates (Yoon et al. 1999). A single sequence only distantly related to Blastococcus saxobsidens (90%) within the Frankineae was detected in Entrance Cave sediment. Several members of the Frankineae including Blastococcus, have been isolated from monuments. Several sequences detected in Entrance sediments were distantly related to the genus Frankia. Frankia sp., are nitrogen-fixing bacteria usually associated with plants. 107 Chapter 3: Results and Discussion .------Bifidobacterium bifidwn S83624 Nocardioi ,..------1.:.P.:.ro~'P:_:ibnibactuium ac""s AB042288 CAV0023 Virgosporangium ochrace1m1 AB006167 MX10039 Micro11wnospori.11.eae Micromonospora chalcea U58S31 Micronwnaspora echinoauranliaca X92618 SL10009 Actinobispora alani,,iphila AF325726 r----- SL10013 Pseudonocardia spinospora Pseudomxarditteae asaccharolytica Actinosyniemma. mirum X84447 Pseudo11ocardineae Saccharothrix violacea AJ24Ui34 u1ur.ea a/bidocapi//ata X84321 lenJuajlavoverrucosus AF183957 .------CAVl312 Crossiella equi AF'245017 Saccharothrix cryophilus AFI 14806 ,----- SL20046 Kibdelosporangium phillipi11ense AJ512464 r-----SE0098 Franldasp. SE10039 I Frankineae Blasrococcus sa:cobJidens AJ316570 0.1 Flgare 3.8: Phylogenetic dendrogram illustrating the evolutionary relationship between cave taxa and members of the Actinomycetaks. The dendrogram was constructed from an alignment of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Bifidobacteriwn bifidum was used as the outgroup species. The scale bar indicates 10% seqnence divergence. Colour Code: Black ; Clone sequences, Blne ; OOGE sequences. Brown ; Isolate sequences 108 Chapter 3: Results and Discussion ~------Biftdobaeterlum bifidum S83624 Cor:mt!bocteritml diptheriae X84248 Tsulcamurelln pourometabola X80628 Tsukomurella stro11djordo.e AF283283 Tsukamurella pulmonis AY254698 ~--- CAVl306 Rhodococcus rltodoclirous X80624 Rilodccoccus erylh"opolls X80618 CAVI203 R11odococc11s globerulus X80619 CAVl104 CAVl321 Corynebacteri11eae Nocardia cummideleus AF430052 Agromyces ro111 os11111 X774'f"/ Agromyces aurantiacus AF389342 Brevibacterium linens AF426135 Brevibacterium iodi.Jam1 X76567 CAVl2S Micrococci11eae Arthrobacter oxydtuJS X83408 '----4 CAV0046 Anhrobacter chlorophe110/icus AF102267 CAVIOOS DMONS Kocurin roscus CAVl117 Brachybactcrium paraco11glc111eralum AJ415377 Braclrybactcriru11 fresconis AJ415378 Bracltvbacterium r/lamnosum AJ41S376 CAVJ31S CAV1002 ~---- Micrococcu.s lylae X80750 ME30023 CAVl318 Arthrobacter pasce11s X80740 0.1 Flgarc 3.10: Phylogenetic dendrogram illustrating the evolutionary relationship between cave taxa and members of the Micrococcineae and Cory11ebacteri11eae. The dendrogram was constructed from an alignment of 1000 nucleotide pooitions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Bifidobacterium bifidwn was used as the outgroup species The scale bar indicates 10% sequence divergence. Colour Code: Black =Clone sequences, Blne = DGGE sequences, Brown = Isolate sequences Figure 3.10 is a phylogenetic dendrogram of the Microccineae and Con;nebacterineae. These bacteria are among the most common organisms isolated from caves. Several strains of Arthrobacter were isolated from cave sediment and moorunilk. One group of Arthrobacter moorunilk isolates were related to Arthrobacter chlorophenolicus (96 % similarity). This is a putatively novel cave species that was also represented in DGGE analysis (DMON4). Arthrobacter is one of the main genera of Micrococcineae, and consists mainly of soil organisms. 109 Chapter 3: Results and Discussion Arthrobacter sp. are remarkably resistant to desiccation and starvation, despite not forming spores and demonstrate considerable nutritional versatility including the ability to decompose a variety of organic compounds. Members of the Arthrobacter have previously been observed in caves demonstrating survival by means of nitrogen fixation or the use of organic substrates as the sole source of carbon and energy, and remain resistant to prolonged periods of nutrient limitation (Barton et al. 2004). A phylotype very closely related to Knoellia subterranea (99%) was detected in sample ME3 and was also isolated from sample ME2. Knoellia sinensis and Knoellia subterranea, were recently isolated from sediment in Reed Flute Cave in China (Groth et al. 2002). Two phylotypes affiliated with the genus Nocardia were detected in sample ME2, ME20019 being almost identical to N.carnea (99%) and ME20104 being more distantly related to N.corynebacteroides (94%) perhaps representing a novel species of the Nocardia. Coryneform bacteria, Nocardia and Rhodococcus, are soil organisms sometimes utilising hydrocarbons. Species of these genera are known to degrade organic matter and are able to decompose environmentally hazardous chemical compounds. Several Nocardia and Rhodococcus sp. were isolated from all sediment and moonmilk samples and although Rhodococcus sp. were not detected in culture-independent analyses. Members of the genus Rhodococcus show a remarkable degree of metabolic diversity and currently are used as whole-cell biocatalysts in several industrial processes (Hughes et al. 1998). Phylotypes affiliated with the Streptomyces were ubiquitous in cave samples (Figure 3.11). Members of the Streptomyces dominated isolations from sediment and moonmilk accounting for approximately 60% of isolates obtained. These isolates represented 10 species of Streptomyces (Table 3.3) The most common species isolated were S. subrutilus and S. caviscabies. S. subrutilus was detected in all sediment, speleothem and moonmilk samples and clones clustering with this lineage were detected in Entrance sediment and calcite mat material, ME2. S. caviscabies was isolated from all samples except for ME2. It was also detected in Loons sediment and moonmilk samples. The genus Streptomyces encompasses a large number of recognised species. Streptomyces are the most common soil bacteria along with the Arthrobacter. Members of the Streptomyces favour alkaline to neutral, well drained soils such as sandy loams or soils 110 Chapter 3: Results and Discussion covering limestone. Limestone caves and lava tube caves often contain wonderful displays of filamentous actinomycetes that may cover entire ceilings and walls of caves giving a 'silvered' appearance (similar to sample ME2). Probably many of the discrete lichen-like colonies frequently noted on walls and formations in the dark zone may be Streptomyces species since they often have the powdery appearance and characteristic earthy odour common to cultures of this genus. Several of the isolates from sediments and moonmilk in this study had this powdery appearance and earthy odour. It has also been suggested that the abundant Streptomyces in caves is probably responsible for the earthy smell of caving (Caumartin, 1963 in Ford & Cullingford, 1976). 111 Chapter 3: Results and Discussion ~------Bifidobacterium bifidum 583624 Streptomyces violaceon1ber AF503492 Streptomyces gougerotii Z76687 Streptomyces mt~ersensis Z16688 ME20041 CAVl314 SEOOSO ----CAVOOIS Streptomyces macrospoms Z68099 Streplomyces beijiangensis AF385681 Streptomyces aureus AY094368 treptomyces microstreptospora AB006l 59 Streptomyces sanglieri AY094364 CAV1231 CAVIOOS Kitasatospora mediocidica U93324 Kitasatospora setae U93332 SL10055 CAVl317 SL10019 Streptomyces virf(iniae 085121 Streptomyces himgiriensis A Y370772 Streptomyces caviscabies AFI 12160 CAV1025 CAVJ116 CAVIOIO CAV1313 CAVIOl9 CAVIOOI 0.1 Figure 3.11: Phylogenetic dendrogram illustrating the evolutionruy relationship between cave taxa and members of the Streptomycineae. The dendrogram was constructed from an alignment of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbour·joining method. Bifidobacterium hifidum was used as the outgroup species. The scale bar indicates I 0% sequence divergence. Colour Code: Black = Clone sequences, Brown = Isolate sequences. 112 Chapter 3: Results and Discussion Four phylotypes were detected clustering within the Actinobacteria but not affiliated with the Actinomycetales. Figure 3.12 is a phylogenetic dendrogram of Actinobacteria subclasses Rubrobacterideae and Sphaerobacterideae and unclassified Actinobacteria. Described members of the Rubrobacterideae are largely thermophilic (eg. Thermoleophilum minutum, Thermoleophilum album, Rubrobacter radiotolerans). Two clones, from moonmilk samples, were loosely affiliated with members of the thermophilic genus Thermoleophilum (89-93%) forming a monophyletic radiation within the Rubrobacterideae and perhaps representing cold-adapted members of this taxa. The Rubrobacterideae are a broad monophyletic group within the Actinobacteria consisting of to date largely uncultivated organisms (Rheims et al. 1996). Culture-independent studies have detected members of this group as ubiquitous and an ecologically significant radiation of the Actinobacteria, inhabiting a diverse array of environments including peat bog (Rheims et al. 1996), forest soil (Liesack & Stackebrandt, 1992), geothermal soil (Fuhrman et al. 1993), paddy and soybean fields (Ueda et al. 1995) and marine habitats (Fuhrman et al. 1993). Within the unclassified Actinobacteria, 2 clones from Entrance sediment, SEl, were distantly related to Candidatus Microthrix parvicella (91 %). Microthrix parvicella is a filamentous organism isolated from an activated sewage treatment plant. One sequence, also from SEl, was loosely affiliated with thermophile Sphaerobacter thermophilus. As confirmed in this study, actinomycetes are the most common and abundant group isolated from caves samples and are detected consistently, though in moderate numbers, in culture-independent studies. Streptomyces species are particularly abundant and in some cases, can be found as apparently monospecific colonies (Arroyo & Arroyo, 1996). A number of actinomycetes isolated from caves have the ability to produce various types of crystals. Studies in Altamira and Tito Bustillo Caves demonstrate that the host-rock (bedrock), cave formations and rock art paintings are coated by dense networks of bacteria, mainly actinomycetes and these bacteria can induce constructive (calcification, crystalline precipitates) and destructive (irregular etching, spiky calcite) fabrics. Because of this ability it has been proposed that these bacteria and others are directly or indirectly involved in constructive biomineralisation processes in caves (Laiz et al. 1999; Barton et al. 2001; Canaveras et al. 2001; Groth et al. 2001; Jones, 2001). Little is 113 Chapter 3: Results and Discussion known concerning the distribution, population dynamics, growth rates and biogeochernical processes of Actinobacteria in caves, in spite of the fact that they seem to constitute a significant part of the "culturable" microbial population of these habitats. A prerequisite for the study of the role of actinomycetes in biogeochemical processes is the isolation and identification of these organisms (Groth et al. 1999a) . .------Tliemroproleus te11a.\ J\!35966 SElOOOl SpllfU'robactl'T'uleae Uncultured bactenwn clone FBP471 AY250886 Conobaccen11111 glomerans X79048 Conobacteruleae Rubrobactendeae RI1brolxwer rad101oleraus U656-f.7 Umdennfied bactenum \\bl...1'06 AF31'Tl69 SE200SO SE10037 Femmurolmmi ac1d1pluhm1 AF251436 l Inclassif1ed Ach11obactena Catliayosporangmm alboflavum AB006158 SE10060 Candi.datus ,\>ficrot1mx pmvicellcr X89774 Pse11do11ocardm tl1ermophila AJ252830 Streptomyce" allmi; X53163 Micromonospora cllf'llcea U58531 Fronkto. sp AF034716 Gfycomyce.s lwrlnnensis AJ293747 Acul1m1crobu11nferrooJ.1da11s U7%47 Actmobactendeae Btfidabaclenum b1fidum S83624 Aclmo111)ce~ buv1sX81061 Micrococcus lylae X80750 Corynebaclena d1pthen.ne X842..J8 Propiombactanum acnes .<\.B042288 __0_1_ Figure 3.12: Phylogeneuc dendrogram tllustratmg the e\•olutmnmy relattonshtp between cave ta'l(a and members of the 4.rtmolwNendeae The dendrograrn was constructed from an ahgnment of 1000 nucleotide pos1tmn'i DIStances were calculated m DNADIST and trees "'ere mferred by the ne1gbbour-J01mng method Thennoproteus tena.x was used as the outgroup species The scale bar md1cates 10% sequence divergence 114 Chapter 3: Results and Discussion Finnicutes Few clones in this study were affiliated with the Finnicutes (low G+C Gram-positive bacteria). A total of five sequences distributed in three phylotypes were detected (Table 3.2). In contrast, 17 moorunilk isolates distributed across seven strains were identified as members of the genera Bacillus, Paenibacillus and Sporosarcina. Figure 3.13 illustrates the phylogenetic relationships of phylotypes and cave isolates to cultivated members of the Firmicutes. Two phylotypes were detected in moomnilk samples. MX10063 was closely related (99%) to Bacillus subtilus, also isolated from samples ME3 and MXl. Remaining Bacillus species isolated include B. simplex, B. pumilus, B. indicus, and B. mycoides, cultured from all moomnilk samples (Figure 3.13). Bacillus sp. are aerobic, endospore forming and mainly found in soil. ME20098 was affiliated with Sporosarcina ureae and strains of this microbe were isolated from sample ME2 and ME3. Members of the genus Sporosarcina are strictly aerobic. S. ureae is common in soils with urea input and is perhaps an important ecological degrader of urea. A single phylotype affiliated with Finnicutes was detected in sediment, SL10009, showing a distant relationship (91%) to Ruminococcus flavescians, usually detected as a symbiont in the gut of animals. 115 Chapter 3: Results and Discussion Ther111oprote11s 1e11a.x !Vf35966 .----- lactobaci/lus delbmeckii M58814 Streptococcus cristalus AY281090 Lactobacillales Streptococcus 1hora/te11sis C/ostridium butyricum AB07S768 Clostridia ~------Mycop/asma mycoides M23943 Mollicutes ~----- Rumi11ococcus jlavescie11s XS.5091 ...------Anaerobic bacterium LR7.2 A Y327251 .....______SL10009 Clostridia Pae11ibacillus polymyxa AJ320493 Pae11ibacillus turice11sis clone B2 AF378699 Pae11ibaci l/11s W\/llllii AJ633647 Pae11ibacillaceae Pae11ibacillus graminis strain RSA19 CAVI309 Geobacillus stearother111ophi/11s strain R-20093 AJ586387 Pla11ococcus cilrea X62172 Sporosarcina 111ac11mrdoe11sis CMS 21 w AJ514408 Permafrost bacteriumDT-ID02 AY378272 Pla11ococcaceae Filibacter limicola AJ292316 Bacil/11s coh 11ii X76437 Bacil/11s /iche11ifor111is X60623 Bacillus pumilus AY456263 CAVl102 Bacillaceae 0.1 Figure 3.13: Phylogenetic dendrogtam illustrating the evolutionary relationship between cave taxa and members of the Fimticutes. The dendrogtam was constructed from an alignment of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbout-joining method. Themwproteus te11ax was used as the outgroup species. The scale bar indicates 10% sequence divergence. Colour Code: Black = Clone sequences. Brown = Isolate sequences. 116 Chapter 3: Results and Discussion ....------Then11oproteus tenaxM35966 .------Chlorobium limicola AJ290824 Chlorobi Bacteroidales .----- SLI0019 Flexibacter tructuosus M.58789 Sphi1111obacteriw11 multivora11 014025 Sphi1111obacteriw11 faeciuJn AJ438176 Sohineobacterium soirilivorw11 014026 Sphingobacteriales Glacier bacterium FJSS AY315161 Uncultured Bacteroidetes bacterium clone Bisi29 AJ318173 CAVI317 Pedobacter heparinus AJ438172 ...------Cryotnorpha ignava AF170738 .----- Arctic sea ice bacteriumARK10177 AF468426 MX10045 ~----- SL10020 Flavobacteria columnare M58781 FlavobacteriuJ11 aquatile M62797 Flc111obacteria ferruginew11 M62798 SL10003 Flat>obacteila limicola AB075230 Flavobacteriales CAVOOlS CAVOOJO Antarctic bacterium R-7933 AJ440987 Bacterium C:Sl 12 AYl24338 C AVI311 F/ll!•obacteria leeana AB180738 Glacier bacterium FJS20 AY315160 Elbe River snow isolate Iso8 AF150713 SL10035 CAV0018 DMON6 0 I Figure 3.14: Phylogenetic dendrogram illustrating the evolutionaiy relationship between cave taxa and members of the Cytoplraga-Flexi.bacter-Bacteroides group. The dendrogram was constructed from an alignment of 1000 nucleotide positions. Distances were calculated in DNADIST and trees were inferred by the neighbour-joining method. Then11oproteus tenax was used as the outgroup species. The scale bar indicates 10% sequence divergence. Colour Code: Black= Clone sequences. Blue = DGGE sequences. Brown = Isolate sequences. CFB Group A total of 65 clones distributed in 14 phylotypes were affiliated with the CFBs (Table 3.2). The CFBs were the second most abundant major phyla detected in moonm.ilk samples ME3 and MX1. Several of these sequences clustered with psychrophilic Flavobacteriaceae (Figure 3.14) that are represented by various aerobic and heterotrophic genera. Several sequences from both samples ME3 and MX1 were closely related to Flavobacteria limicola (98%) a psychrophilic, organic polymer degrader (Tama.ki et al. 2003). This phylotype was present in DGGE analysis 117 Chapter 3: Results and Discussion and represented 10-12% of the total diversity sampled in the moonmilk clone libraries, demonstrating its dominance in these habitats. A novel Flavobacteria sp. was isolated from moonmilk sample ME3 clustering with the F. leeana-Iike sequences. A single sequence MX10045 showed distant similarity (92%) to Cryomorpha ignava a cold-adapted, strict aerobe isolated from Antarctic quartz stone subliths (Bowman et al. 2003). Phylotypes ME30011 and MON0015 from moonmilk clustered with psychrophilic members of the Sphingobacteriales, genera Sphingobacterium and Pedobacter (Figure 3.14). Phylotype ME30011 represented by three clones was related to Pedobacter cryconitis, a facultative psychrophile isolated from an alpine glacier (Margesin et al. 2003). Phylotype MON0015 was affiliated with Sphingobacterium faecium. A number of uncultured glacier and sub-glacial sediment clones (FJS and FX clone groups) clustered with moonmilk phylotypes identified in this study, inferring the presence of cold adapted taxa in these samples. Three phylotypes clustered within the Bacteroides group. SL0019 branched with Flexibacter tructuosus (92% sequence similarity). Phylotype CAV0026, detected in sediment and moonmilk samples from Entrance Cave, is distantly related to uncultured Bacteroides bacterium Mo-0.2plat-K3, detected in freshwater. Phylotype SL10028 was not closely affiliated with any described taxa, however it clustered with a group of uncultured bacterial clones from Palaeolithic rock art in Spanish and Italian caves within the Bacteroides clade (Figure 3.14). The Bacteroides group includes a mixture of physiological types such as strictly anaerobic Bacteroides and aerobic gliding bacteriCJ. such as Flexibacter. Bacteria with gliding motility have no flagella but are able to move when in contact with surfaces. Acidobacteria A total of 11 clones affiliated with the Acidobacteria were detected in the cave samples. Most clones form a monophyletic clade within sub-Phylum A of the Acidobacteria showing varying degrees of similarity to uncultured bacterium DA008 (90-94%), a clone from grassland soils (Figure 3.15). These sequences were retrieved from moonmilk samples, particularly sample ME2 (5 clones). The remaining sequences were affiliated with Ellin isolates from Australian soils 118 Chapter 3: Results and Discussion (Sait et al. 2002; Joseph et al. 2003) within sub-Phyla C and D. Though the Ellin group represents cultured members, these have not been described to date thus no information is available about their physiology or metabolism. The Acidobacteria are a relatively cosmopolitan group, widely distributed in the environment though in general are highly correlated with the soil habitat. (Hugenholtz et al. 1998). The division was defined by Ludwig et al. (1997) on the basis of cloned 165 sequences from soil, freshwater sediments and activated sludge in many geographic locations and its members are thought to be ecologically significant in many ecosystems. However it is a poorly studied division thus far, consisting of only a few cultured representatives: Acidobacterium capsulatum an acidophilic chemoorganotroph from acid mineral environment (Kishimoto et al. 1991), Geothrix fermentans an iron-reducing bacteria from a hydrocarbon contaminated aquifer (Coates, 1999), and Holophaga foetida a homoacetogenic bacterium degrading methoxylated aromatic compounds (Liesack et al. 1994). 119 Chapter 3: Results and Discussion r------Then11oproteuste11a.\1-135966 Bactenal speaes (clone 11-14) Z95710 '----- SL10020 Sub-Phyla D 4.c1dolXlcler11m1 capsulalum D26171 Bactenwn Ellm5289 AY23-l6-IO Bactenwu Bhn6CT75 AY234727 ME20020 Sub-PhylaC Uncultured bactenum clone Alt9-h."71 AJ421902 Uncultured bactenum cloneC11-K25AJ421117 SL20005 ~---- Uncultured bactenum clone Alt9-K74 AJ..J.21904 Bactenum Elhn6100 AY234752 Baclenmn Elhn6071 AY234723 Geot/lru .frrme11ta11s U41563 Holophagafoeluia X77215 Sub-Phyla B '------Uncultured bactenwn clone C'4-K19 AJ421210 llncultured bac1emnn DA008Y112597 Sub-Phyla A MONOIJ.J5 Uncultured bactemun clone C2-K16 AJ421198 ME20013 01 Figure 3.15': Phylogenetic dendrogram 1llustratmg the evoluuonary relat10nsh1p between cave ta\.a and members of the Ac1dobacterza The dendrogram was con;tructed from an alignment of 1000 nncleoude posmons Distances were calculated m DNADIST and trees were mferred by the ne1ghlxmr-Jommg method Themioproteus temv.. \\"1\S used as the outgroup species The scale bar md1cates 10% sequence dn ergence 120 Chapter 3: Results and Discussion Planctomycetales A total of 31 clones affiliated with the Planctomycetales were detected in sediment and moorunilk samples (Figure 3.16). The majority of these clones belonged to six deeply branching phylotypes within the genera Planctomyces, Pirellula and Gemmata, showing distant (87.2-90% similarity) relationships to cultured members. This is not suprising as the intralineage phylogenetic depth of the Planctomycetales was recently expanded to 30.6% (Chouari et al. 2003). One phylotype (SED0047) detected in all sediments, was closely related to Pirellula staleyi (96%). Four cultured genera, consisting of seven species overall, have been described to date, Planctomyces, Pirellula, Gemmata and Isophaera (eg. Schlesner, 1986; Giovannoni et al. 1987; Schlesner 1989). All these organisms are aerobic chemoheterotrophs. Knowledge of this group is limited because of the relatively few species that have been obtained in pure culture. Membership of the planctomycete group has been extended not only to chemoorganotrophs and obligate or facultative aerobes but also to obligate anaerobes, autotrophs and phototrophs, demonstrating diverse metabolic properties within this line of descent (Fuerst, 1995; Miskin et al. 1999). For example, a planctomycete was found to be responsible for anaerobic oxidation of ammonia (Strous et al. 1999). All Planctomycetales were originally isolated from aquatic habitats as diverse as acid bogs and sewage treatment plants though culture-independent studies have revealed the presence of Planctomycetales in more diverse environments including marine, sediment, anoxic bioreactors, anoxic sediments and caves (DeLong et al. 1993; Godon et al. 1997; Holmes et al. 2001; Tay et al. 2001; Chouari et al. 2003). The Planctomycetales were a significant component of Entrance Cave dry sediment being the third most abundant group detected in sample SEl (22.5%) whereas in all other samples they constituted a relatively minor component of the community (1-8%). 121 Chapter 3: Results and Discussion ..------T1wmzoproteus tmaxM35966 -----Pla11ctomvccs bras1lie11srs AJ231190 '-----Planctom:yces marts AJ2.o1184 ~---SED0062 '----sE10039 ~---- Pirellu/a sta/eyz AJ23 WB Planctomycetales Uncultured scnl bactenum PRR-7 A T390478 Uncultured soil bactenum PRR-47 AJ390484 Uncultured s01l bactemlll.l PRR-8 A..1390-1-79 r------Bactenum (s01l clone MCl 1) X64378